Thermo Fisher Scientific Genescan® Reference guide

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Thermo Fisher Scientific Genescan® Reference guide | Manualzz
GeneScan Reference Guide
®
Chemistry Reference for the ABI PRISM® 310
Genetic Analyzer
© Copyright 2000, Applied Biosystems
For Research Use Only. Not for use in diagnostic procedures.
ABI PRISM and its Design, Aquapore, AmpliCover, Anitron, Biobytes, Brownlee, FastPhoramidite, GeneScan, Genotyper, HLP, INHERIT, MicroAmp, MicroCoat,
MPLC, NEWGUARD, ONESTEP, OPC, PCR-MATE, Phosphalink, POLYPORE, Precipitette, ProBlott, PROCISE, ProFocus, ProSort, ProSpin, SeqEd, Sequence
Navigator, SPHERI5, SPHERI10, StockMarks, Stretch, Synergy, SynthAssist, and VeloSep are registered trademarks of PE Corporation or its subsidiaries in the U.S.
and certain other countries.
ABI, ABI Masterpiece, Applied Biosystems, AutoAssembler, BaseSprinter, CATALYST, GeneAssist, LV40, MatchMaker, PDQ, Primer Express, and ProSorb are
trademarks of PE Corporation or its subsidiaries in the U.S. and certain other countries.
AmpErase, AmpliTaq, AmpliTaq Gold, AmpliType, AmpliWax, EnviroAmp, GeneAmp, QuantiBlot, TaqMan, and UlTma are registered trademarks of Roche
Molecular Systems, Inc.
Apple, AppleTalk, AppleScript, Macintosh, and Power Macintosh are registered trademarks of Apple, Inc.
AFLP is a trademark of Keygene N.V.
ABI, ABI PRISM, AmpFl STR, AmpFl STR Blue, AmpFl STR Green, Applied Biosystems, MicroGel, POP, POP-4, Primer Express, Profiler, Profiler Plus, and True
Allele are trademarks of PE Corporation or its subsidiaries in the U.S. and certain other countries.
All other trademarks are the sole property of their respective owners.
P/N 4303189B
Contents
1 Introduction. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 1-1
Using This Manual . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 1-1
Technical Support . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 1-3
2 Experimental Design Considerations. . . . . . . . . . . . . . . . . . . . . . 2-1
Using GeneScan Analysis Software to Analyze DNA Fragments . . . . . . . . . . . . . . . . . . . . . . . 2-1
Working with Multiple Colors . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-2
Choosing Fluorescent Labeling Methods. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-5
Determining Loading Concentrations for Samples . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-8
Optimizing Electrokinetic Injection Parameters. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-9
Optimizing Electrophoresis Conditions . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-13
Using Control DNA . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 2-16
3 General Analysis and Evaluation Techniques . . . . . . . . . . . . . . . 3-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 3-1
Analyzing the Data . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 3-2
Evaluating Data Quality . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 3-8
Quantitating Nucleic Acids. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 3-10
Evaluating Matrix Quality . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 3-11
4 ABI PRISM Dyes . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 4-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 4-1
Available Dyes . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 4-2
Understanding Dye Spectra . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 4-3
Choosing Dye/Filter Set Combinations . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 4-5
Emission Spectra for Representative Dye/Virtual Filter Set Combinations. . . . . . . . . . . . . . . . 4-8
5 Sizing and Size Standards. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-1
Introduction to Sizing . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-2
Preventing/Troubleshooting Sizing Problems . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-5
GeneScan Internal Lane Size Standards. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-7
GeneScan-350 Size Standard . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-8
GeneScan-400HD Size Standard . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-10
GeneScan-500 Size Standard . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-12
i
GeneScan-1000 Size Standard. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-14
GeneScan-2500 Size Standard. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 5-16
6 Optimizing PCR . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-1
Choosing Reaction Volumes and Tube Types . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-2
Designing Custom Primers . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-3
Determining Reagent Concentrations . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-6
Choosing the Right Enzyme . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-8
Multiplexing PCR . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-10
Using RNA Templates . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-12
Preventing Competing Side Reactions—Hot Start PCR . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-13
Modifying Thermal Cycling Parameters . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-15
Avoiding Contamination . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-16
3´ A Nucleotide Addition. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-18
Stutter Products . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-21
Preparing PCR Products for Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 6-23
7 SSCP Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-1
Introduction to SSCP Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-2
Before You Begin. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-3
PCR Amplification, Labeling, and Controls . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-4
To Save Time—Prerun Checklist. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-7
Preparing for a Run . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-8
Analyzing the Data . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-12
Optimizing SSCP Run Conditions. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-14
Troubleshooting . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 7-17
8 Microsatellite Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-1
Introduction to Microsatellite Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-2
Before You Begin. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-3
PCR Amplification, Labeling, and Controls for Microsatellite Analysis . . . . . . . . . . . . . . . . . 8-4
To Save Time—Prerun Checklist. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-6
Preparing for a Run . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-7
Analyzing the Data, Part I—Using GeneScan. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-10
Analyzing the Data, Part II—Allele Binning Using Genotyper 2.0 . . . . . . . . . . . . . . . . . . . . 8-12
Troubleshooting Microsatellite Analysis . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 8-25
ii
9 Microsatellite Analysis Applications. . . . . . . . . . . . . . . . . . . . . . . 9-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-1
Microsatellite Analysis Using the LMS V2 . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-2
Troubleshooting the LMS V2 . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-4
LOH Screening. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-5
Performing LOH Screening . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-7
RER Screening . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-13
Troubleshooting LOH and RER Screening . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-16
Animal Paternity. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-17
Human Identification . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 9-19
10 AFLP Mapping . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 10-1
Introduction . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 10-1
The AFLP Technique . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 10-5
11 Troubleshooting . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 11-1
Troubleshooting PCR Amplification . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 11-1
Troubleshooting PCR Product Detection . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . 11-7
A Reagent Preparation . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . A-1
B Creating Matrix Files . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . B-1
Creating the GeneScan Matrix File . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .B-1
C Preparing 5´-End Labeled Primers . . . . . . . . . . . . . . . . . . . . . . . C-1
Overview . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .C-1
Introduction to 5´-end Labeling . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .C-2
Instrument Setup. . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .C-4
Synthesis and Purification of 5´-end Labeled Primers . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .C-6
Calculating Absorbance for DNA Samples . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .C-10
D References . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .D-1
iii
E Part Numbers . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . E-1
ABI PRISM DNA Fragment Analysis Kits and Reagents. . . . . . . . . . . . . . . . . . . . . . . . . . . . . .
ABI PRISM 310 Genetic Analyzer . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .
Reference Materials . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .
Updates . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . . .
Index
iv
E-1
E-5
E-7
E-8
Introduction
1
1
Using This Manual
How This Manual Is This manual contains four major topic divisions:
Organized ♦ General knowledge (Chapter 2 through Chapter 6):
♦
♦
♦
–
Designing experiments
–
Analyzing and evaluating data
–
Fluorescent dyes and recommended dye sets
–
Choosing size standards and size-calling methods and troubleshooting sizing
problems
–
Optimizing PCR
Applications (Chapter 7 through Chapter 10):
–
SSCP analysis protocols and optimization suggestions
–
Generic microsatellite analysis protocols and optimization suggestions
–
Specialized applications of microsatellite analysis
–
Information about AFLP™ microbial fingerprinting and plant mapping
applications
Troubleshooting (Chapter 11):
–
PCR amplification
–
PCR product detection
Appendices (A through E):
–
Reagent preparation
–
Preparing 5´-end labeled primers
–
Creating matrix files
–
Literature references
–
Part numbers
continued on next page
Introduction 1-1
Conventions Used in The following words and styles draw your attention to specific details of the
This Manual information presented in this manual:
Note
A note calls attention to useful and/or interesting information.
IMPORTANT
experiments.
This information is emphasized because it is critical to the success of your
! WARNING ! Indicates that physical injury to yourself or others could result if you
do not follow the recommended precautions.
Safety Information For information on the safe operation of the ABI PRISM® 310 Genetic Analyzer, refer to
the ABI PRISM 310 Genetic Analyzer Site Preparation and Safety Guide (P/N 903558).
Updates Visit our World Wide Web site (www.appliedbiosystems.com/techsupport) for updates
to this manual.
Other Manuals This manual is designed to be used in conjunction with the following manuals:
1-2 Introduction
♦
ABI PRISM 310 Genetic Analyzer User’s Manual (P/N 903565)
♦
GeneScan® Analysis Software User’s Manual (P/N 904435)
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Introduction 1-3
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Introduction 1-5
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1-6 Introduction
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Introduction 1-7
Experimental Design
Considerations
2
2
Using GeneScan Analysis Software to Analyze DNA Fragments
Introduction The GeneScan® Analysis Software analyzes the data collected by the ABI PRISM 310
Genetic Analyzer to size and quantitate DNA fragments. GeneScan analysis of
sample files includes establishing a baseline, adjusting for spectral overlap of the
dyes, peak detection, and size calling.
The GeneScan Analysis Software sizes and quantitates DNA fragments automatically,
allowing faster and more accurate analysis than traditional methods such as
radiolabeling. Depending on your run conditions, you can achieve resolution sufficient
to differentiate between fragments that have apparent sizes up to 5000 base pairs.
When you use the GeneScan system, you can label different DNA fragments with up
to three different color fluorescent dyes. A fourth color is reserved for the GeneScan
Internal Lane Size Standard. The size standard is used for precise size calling without
the problems often encountered using other techniques, such as band-shift artifacts
and run-to-run variation.
You can display the results of an experiment as electropherograms, as tabular data, or
as both. Electropherograms show fluorescence intensity as a function of fragment size
or migration time. Each electropherogram represents a single injection. The tabular
data provides precise sizing and quantitative information. The data can be exported to
downstream applications, such as Genotyper® software.
In This Chapter This chapter summarizes the basic design factors that you should consider before
beginning any GeneScan fragment analysis experiment.
This chapter contains the following topics:
Topic
See Page
Working with Multiple Colors
2-2
Choosing Fluorescent Labeling Methods
2-5
Determining Loading Concentrations for Samples
2-8
Optimizing Electrokinetic Injection Parameters
2-9
Optimizing Electrophoresis Conditions
2-13
Using Control DNA
2-16
Experimental Design Considerations 2-1
Working with Multiple Colors
Introduction Fluorescent labeling enables you to analyze many independent loci in the same
capillary injection, using color in addition to size to distinguish between fragments. To
take advantage of this, you need to consider more factors than you would with
traditional techniques.
Guidelines For Performing Any Experiment
You should always:
♦
Use the same GeneScan Internal Lane Size Standard labeled with the same dye
for all samples in a single study.
♦
Compare peak areas, heights, and sizes in nucleotide bases only for fragments
that are labeled with the same dye.
For example, compare FAM-labeled fragments only to other FAM-labeled
fragments.
Note
It is possible to compare samples labeled with different dyes when comparing relative
sizes and peak height and area ratios.
For Working with Similarly Sized DNA Fragments
If the sizes of different fragments overlap, then you can do one of the following to
differentiate between them:
♦
Label overlapping products with different dye colors.
♦
Choose new primer sites to alter the PCR-product fragment lengths.
♦
Load overlapping products during different capillary injections.
Multiplexing to To exploit the potential for increased throughput using ABI PRISM™ multicolor
Increase fluorescent dye technology, you will want to multiplex electrophoresis by co-loading
Throughput the products of multiple PCR reactions in the same capillary injection. Depending
upon your application you may also want to multiplex the PCR.
Co-electrophoresis
Before performing PCR for co-electrophoresis, be sure that you follow these
guidelines:
♦
Use different dye labels for PCR reactions with overlapping product sizes.
♦
Use a combination of dyes that display in different colors and can be detected by
the same virtual filter set.
Table 4-3 on page 4-6 lists recommended filter/dye set combinations.
♦
Use greater dye concentrations in PCR reactions with dyes of low emission
intensity than for dyes of high emission intensity. (See “Accounting for Differences
in Dye Signal Strengths” later in this section.)
After pooling PCR products, you may need to perform a desalting step prior to loading
samples. Pooling products from multiple PCR reactions often increases the salt
concentration in the loaded samples. (See “Decreasing the Salt Concentration” on
page 2-3.)
2-2 Experimental Design Considerations
Multiplexing PCR
You can multiplex the PCR by combining more than one pair of primers in the same
PCR reaction tube. Do not multiplex primers with similar product lengths labeled with
similar dyes.
Note
For microsatellite applications, do not multiplex primers labeled with the same
fluorescent dye for loci with overlapping allele size ranges. If you do not know the full extent of
the allele size ranges leave at least 15–20 base pairs between the known size ranges.
Before performing the PCR, perform a preliminary check for primer compatibility.
Avoid excessive regions of complementarity among the primers. Also, choose primer
pairs with similar melting temperatures. For more information on primer-pair
compatibility, see “Designing Custom Primers” on page 6-3.
After identifying compatible primer pairs, test the pairs for successful co-amplification.
You will often need to optimize reaction conditions and, occasionally, you will need to
redesign the primers. For more information on optimizing reaction conditions, see
“Multiplexing PCR” on page 6-10.
Ensuring Adequate Accounting for Differences in Dye Signal Strengths
Signal Intensity The intensity of emitted fluorescence is different for each dye. For example, to
generate signals of equal intensity you need to load approximately eight times as
much ROX as you do 6-FAM or TET.
The following lists ABI PRISM dyes in order of increasing emission intensity when
excited by the dual-mode argon laser:
♦
ROX (lowest signal strength)
♦
TAMRA
♦
HEX
♦
JOE, NED
♦
5-FAM, 6-FAM, TET (highest signal strength)
See Chapter 4 for more information about ABI PRISM dyes, dye spectra, and the argon
ion laser.
Decreasing the Salt Concentration
Salt anions compete with negatively charged DNA for entry into the capillary during
electrokinetic injection. As the salt concentration increases, less DNA enters the
capillary, weakening the signal. Excess salt can also precipitate the DNA in the
sample tube in the presence of formamide.
You might be able to compensate for the decreased signal intensity by increasing the
sample injection time and/or injection voltage. If this does not work you will need to
desalt and concentrate the samples.
To desalt:
♦
Use an Amicon Centricon-100 (or Centricon-30 for fragments smaller than 130
base pairs in length) Microconcentrator.
♦
Precipitate the pooled PCR product and resuspend in distilled, deionized water.
Experimental Design Considerations 2-3
♦
Dialyze the sample on a filter membrane to remove salt from the solution:
Step
Action
1
Float a Millipore VS filter (Millipore P/N VSWP 02500), shiny side up, on top of
50 mL of deionized, autoclaved water in a 50-mL conical plastic tube.
2
Carefully spot approximately 15 µL of sample on top of the filter, using an
appropriate pipette. Dialyze the sample for 20 minutes.
3
Using a pipette, very carefully remove the sample and dilute.
Note
Do not increase sample concentration by evaporating the samples without performing
a desalting step. This increases the salt concentration, making it more difficult to denature the
DNA and decreasing the signal strength.
Adjusting the Signal Intensity
For more information on adjusting the signal intensity see “Determining Loading
Concentrations for Samples” on page 2-8 and “Optimizing Electrokinetic Injection
Parameters” on page 2-9.
2-4 Experimental Design Considerations
Choosing Fluorescent Labeling Methods
\
Recommended Most GeneScan applications analyze PCR products. You can use either of two
Methods fluorescent labeling methods during PCR amplification:
♦
Incorporating a 5´-end labeled primer during the primer-annealing step
♦
Incorporating fluorescent dye-labeled dUTPs or dCTPs ([F]dNTPs) during the
primer-extension step
IMPORTANT
With any labeling technique you should use only ABI PRISM dyes. Other dyes,
or mixed isomers of dyes, have variable spectral shifts that will interfere with making a
multicomponent matrix. (The matrix compensates for the spectral overlap between the dyes.)
[
Comparing Labeling Advantages of Using 5´-end Labeled Primers
Methods ♦ High precision
All fluorophores affect DNA mobility to some degree. Different fluorophores have
different mobilities. Because fragments labeled with 5´-end labeled primers have a
single fluorophore at the 5´ end, the mobility of all detectable fragments is
comparably affected. Therefore, fragment peaks tend to be narrow.
By contrast, fragments labeled with [F]dNTPs have a variable number of
fluorophores attached in variable positions on both strands. Thus, peaks tend to
be wider with [F]dNTPs, and can appear to be split.
♦
Consistent quantitation
Every fragment in a peak contributes a single fluorophore to the total signal. Thus
peak area is directly proportional to the number of molecules. A population of
fragments labeled with [F]dNTPs has a variable number of attached fluorophores.
(The average number of attached fluorophores depends upon the fragment’s base
composition and length and upon the ratio of [F]dNTPs to dNTPs added to the
reaction mixture.) Thus it is inadvisable to compare peak areas between
fragments labeled with [F]dNTPs.
♦
Distinguishing between the forward and reverse strands
By attaching a different fluorophore to the forward and reverse primers, you can
distinguish the peaks corresponding to the forward strand, the reverse strand, and
residual double-stranded product.
Advantages of Using [F]dNTPs
♦ High sensitivity
Because most fragments contain multiple fluorophores, a given number of
[F]dNTP-labeled fragments will produce a greater signal than the same number of
5´-end labeled fragments. The increased signal strength allows you to use smaller
reaction volumes and fewer amplification cycles during PCR.
♦
Low cost
You can add [F]dNTPs to any PCR reaction. You do not need to order or
synthesize fluorescently-labeled primers before each PCR and you can use
[F]dNTPs with your existing primer sets.
Experimental Design Considerations 2-5
♦
Post-PCR end-labeling
Post-PCR end-labeling with [F]dNTPs using Klenow is an alternative to labeling
during PCR. See Iwahana et al. (1995) and Inazuka et al. (1996) for details.
You can also label with [F]dNTPs using traditional techniques such as random
priming or nick translation.
Figure 2-1 and Figure 2-2 compare the results obtained using 5´-end labeled primers
and [F]dNTPs. 5´-end labeled primers give better resolution, but [F]dNTPs give better
sensitivity. Note also the unincorporated fluorescently-labeled nucleotides in the
[F]dNTP-labeled sample (bottom panel of Figure 2-1).
Figure 2-1 Results from 5´-end labeling (top) and [F]dNTPs (bottom)
Figure 2-2 Expanded view of the electropherogram from Figure 2-1, showing the differences
in resolution and peak height between the two labeling methods
continued on next page
2-6 Experimental Design Considerations
e
For More You can obtain custom 5´-end labeled primers from the Applied Biosystems Custom
Information Oligonucleotide Synthesis Service either by phone (800-345-5224), by e-mail
([email protected]), or online
(www.appliedbiosystems.com/techsupport).
For information on synthesizing 5´-end labeled primers, see Appendix C.
For information on labeling with [F]dNTPs, consult the [F]dNTP Reagents Protocol
(P/N 402774).
Experimental Design Considerations 2-7
Determining Loading Concentrations for Samples
Why Problems Arise Using too little or too much sample can cause problems. Your ABI PRISM® instrument
can convert a limited range of fluorescent signal into digital values. For optimal results,
you should keep the fluorescent signal between approximately 150 and 4000 relative
fluorescent units (RFU).
Too Little Signal
Below this range, the signal-to-noise ratio is too low to discriminate between sample
peaks and background fluctuations.
Too Much Signal—The Most Common Problem
Above this range, the instrument cannot measure the true value of the signal and
consequently cannot compensate for the spectral overlap among the dyes. As a
result, artifact peaks (called “bleedthrough” or “pull-up” peaks, see page 3-11) can
appear in other colors. Artifact peaks can corrupt both automated size-calling (extra
peaks in the size standard color) and the analysis of co-loaded samples.
How to Proceed ♦
Typically, dilute 1 µL of each PCR product and 0.5 µL of the GeneScan Internal
Lane Size Standard (see Chapter 5), in 12 µL of distilled, deionized water (for
non-denaturing applications) or deionized formamide (for denaturing
applications).
! WARNING ! CHEMICAL HAZARD. Formamide is a known teratogen. It can cause
birth defects. Wash thoroughly after handling formamide. Obtain a copy of the MSDS
from the manufacturer. Wear appropriate protective eyewear, clothing, and gloves. Wash
thoroughly after handling formamide.
♦
If you anticipate an extremely high sample concentration, run dilutions of the
sample as a precautionary measure. If the signal is too strong, you can further
dilute the sample or you can decrease the sample injection time and/or injection
voltage.
♦
If the signal is too weak, first try increasing the signal by increasing the sample
injection time or voltage.
Note
To optimize the signal intensity for a given sample, inject the same sample multiple
times using a range of injection parameters.
♦
If the signal intensity is still too weak or the resolution is poor, concentrate the
sample (see “Decreasing the Salt Concentration” on page 2-3).
♦
If the signal intensity is too low after concentration, see “Problems with Signal
Strength and Quality” on page 11-10 or “Problems with Poor Amplification” on
page 11-1.
2-8 Experimental Design Considerations
Optimizing Electrokinetic Injection Parameters
Introduction Optimizing electrokinetic injection parameters can greatly improve data quality,
run-to-run precision in sizing, and reproducibility in the amount of sample loaded. The
goal is to inject sufficient DNA to yield peaks of adequate height (that is, data with a
good signal-to-noise ratio) while maintaining the resolution and precision required by
the application.
The ABI PRISM® 310 run modules have preset values for injection times and voltages.
These values are adequate for many applications. However, you should consider
modifying the injection parameters if the signal is too strong or too weak or if the
resolution is poor. (The maximum recommended injection time is 30 seconds and the
maximum possible injection voltage is 15 kV.)
When selecting values for injection parameters, consider the following:
♦
The range of fragment lengths
♦
The resolution required
Definition of The resolution, Rs, of two peaks in an electropherogram is defined as follows:
Resolution
P –P
1
2
R s = ---------------------------------------0.5 × ( W 1 + W 2 )
where the Pi are the peak positions measured below the peak apex and the Wi are the
peak widths measured at half peak maximum.
Modifying Injection When you modify the injection time, you will encounter a tradeoff between increasing
Time signal strength and increasing resolution.
Effects on Signal Intensity
For the range of parameter values and sample concentrations used in most
experiments, the signal strength (as measured both by peak height and by peak area)
increases linearly with increasing injection time.
However, as shown in Figure 2-3 and Figure 2-4 on page 2-10, it is not true that an
n-fold increase in injection time results in an n-fold increase in peak height. No
improvement is seen after 10 seconds for the larger fragment. The signal decreases
dramatically after 40 seconds for the smaller fragment. As the injection time increases,
the resolution decreases (Figure 2-5 on page 2-11), leading to increasing peak widths
and decreasing peak heights.
Experimental Design Considerations 2-9
Figure 2-3 Peak height vs. injection time for two different-sized fragments (90 bp and 300 bp)
Figure 2-4 Peak area vs. injection time for two different-sized fragments (150 bp and 340 bp)
Effects on Resolution
Increasing the injection time decreases the resolution. As shown in Figure 2-5 on
page 2-11, the deleterious effect on resolution is more pronounced for larger
fragments.
The decrease in resolution results from an increase in peak width (as opposed to a
decrease in peak separation).
2-10 Experimental Design Considerations
Figure 2-5 Resolution vs. injection time for different-sized fragments
Modifying Injection No trade-off between increasing signal strength and increasing resolution exists when
Voltage modifying injection voltage. Resolution with injection voltages of 319 V/cm (the highest
possible setting) is often indistinguishable from resolution with injection voltages of
53 V/cm. However, lower voltages, which produce lower currents, are often preferable
because injection timing is more accurate. Accurate timing ensures reproducibility in
sample loading.
Effects on Signal Intensity
Peak height and peak area increase linearly with increasing injection voltage.
Figure 2-6 below and Figure 2-7 on page 2-12 show the effect of increasing the
injection voltage from 53 V/cm to 319 V/cm on peak height and peak area,
respectively, for two different-sized fragments.
Figure 2-6 Peak height vs. injection voltage for two different-sized fragments (150 bp and
340 bp
Experimental Design Considerations 2-11
Figure 2-7 Peak area vs. injection voltage for two different-sized fragments (150 bp and
340 bp
Effects on Resolution
Injection voltage has little effect on peak resolution (Figure 2-8).
Figure 2-8 Resolution vs. injection voltage for different-sized fragments
Figure 2-5 on page 2-11 and Figure 2-8 above show calculated Rs values over
increasing injection time and electric field. The plots measure single nucleotide
intervals in the 160-bp and 360-bp ranges. An Rs value of 1 corresponds to fragments
that can be discriminated by one nucleotide.
If Results Are Poor If after adjusting the electrokinetic time and voltage, the signal is still too weak or the
resolution is poor, you may need to concentrate or desalt the sample (see page 2-3).
Setting For information on setting electrokinetic injection values, see the ABI PRISM 310
Electrokinetic Genetic Analyzer User’s Manual.
Injection Values
2-12 Experimental Design Considerations
Optimizing Electrophoresis Conditions
Introduction Optimizing electrophoresis conditions (run time, run voltage, and run temperature)
can greatly improve data quality, run-to-run precision, and/or throughput. When
selecting values for these parameters, consider the following factors:
♦
Range of fragment lengths
♦
Required degree of resolution
♦
Type of genetic analysis you will be performing
For example, does the application require native or denaturing conditions?
The preset electrophoresis parameters in the application modules are set to ensure
the following:
♦
Detection of all fragments in the typical size range permitted by the application
For example, microsatellite loci are rarely over 400 base pairs in length.
♦
Acceptable run times
♦
Acceptable resolution
Modifying Run Time Determining Required Run Time
To determine the minimal acceptable run time for a given run voltage, you will need to
perform a trial run. To ensure that you collect sufficient data to perform analysis, set
the electrophoresis run time approximately 10% higher than the migration time of the
largest fragment of interest.
Note
The “largest fragment of interest” will most probably be a size-standard peak that is
needed for sizing the largest sample fragments of interest. The set of size-standard peaks that
GeneScan uses to generate the sizing curve can vary with the size-calling method. In general,
be sure to include the two size-standard peaks immediately larger than the largest sample
fragment of interest.
Decreasing Run Time
For faster run times, you can increase the electrophoresis voltage, but this can
decrease the resolution.
continued on next page
Experimental Design Considerations 2-13
Modifying Effects on Fragment Migration Rates
Run Voltage Figure 2-9 shows the effect of electrophoresis voltage on migration time. Higher
voltages give faster run times but can affect the resolution (Figure 2-10).
Figure 2-9 Migration time to detector vs. electrophoresis voltage for 204-bp and 5117-bp
GeneScan-2500 fragments, 2.5% GeneScan Polymer in 41-cm capillary at 30 °C
Effects on Resolution
Figure 2-10 shows the effect of increasing electrophoresis voltage on resolution. In
general, resolution is better at lower field strengths.
Figure 2-10 Resolution vs. electrophoresis voltage for different-sized GeneScan-2500
fragments, 2.5% GeneScan Polymer in 41-cm capillary at 30 °C
2-14 Experimental Design Considerations
When to Increase Voltage
If the fragments of interest are well separated or if you need a quick answer, you can
increase the voltage.
Modifying Perform native applications and non-denaturing applications, such as SSCP, at lower
Electrophoresis temperatures (27–42 °C).
Temperature
™
Protocols for most denaturing applications using the POP-4
run temperature.
polymer specify a 60 °C
Laboratory The laboratory temperature should be maintained between 15 and 30 °C. Once the
Temperature and ABI PRISM 310 Genetic Analyzer is set up and in operation, the laboratory
Humidity temperature should not fluctuate more than ±2 °C. The instrument can tolerate up to
80% non-condensing relative humidity. Avoid placing it near heaters or cooling ducts.
For More For information on setting electrophoresis parameters, see the ABI PRISM 310 Genetic
Information Analyzer User’s Manual.
Experimental Design Considerations 2-15
Using Control DNA
Purpose of Control DNA:
Control DNA ♦ Serves as a positive control for troubleshooting PCR amplification
Knowing whether the control DNA amplifies will allow you to distinguish between
problems with the sample DNA (the control DNA amplifies but samples do not)
and problems with reagents, thermal cyclers, or protocols (the control DNA does
not amplify).
♦
Allows you to monitor sizing precision
Because the control DNA is not used to calculate the sizing curve, you can use
the sizes obtained during different capillary injections to verify that sizing precision
(reproducibility) is within acceptable limits.
♦
Guidelines for Use ♦
♦
Allows you to correlate the fragment sizes that you obtain with the fragment sizes
obtained by others, e.g., for the CEPH families in the Linkage Mapping Set
Amplify at least one control DNA sample in every PCR run.
Include at least one injection of amplified control DNA during every capillary run.
Use more than one injection if you vary the electrophoresis parameters during the
run.
CEPH 1347-02 In addition to the GeneScan Internal Lane Size Standards, Applied Biosystems sells
Control DNA the CEPH 1347-02 standard used to generate the Généthon map of the human
genome (P/N 403062).
2-16 Experimental Design Considerations
3
General Analysis and
Evaluation Techniques 3
Overview
In This Chapter This chapter will help you evaluate and analyze data obtained on the ABI PRISM® 310
Genetic Analyzer. In particular, it should help you avoid many common causes of poor
quality data.
This chapter contains the following topics:
Topic
See Page
Analyzing the Data
3-2
Evaluating Data Quality
3-8
Quantitating Nucleic Acids
3-10
Evaluating Matrix Quality
3-11
General Analysis and Evaluation Techniques 3-1
Analyzing the Data
Process Overview The following diagram summarizes the data analysis process using the GeneScan
Analysis software.
Open the project file
Install a new matrix if necessary
Set the Analysis Parameters
Define the size standard
Analyze the data
Analyze Sample
To analyze sample files:
Files
Step
Action
1
Launch the GeneScan Analysis Software.
2
Assign the matrix file to the sample files if you have not already done so in the
ABI PRISM 310 Collection Software.
Note
For detailed instructions see “Assigning a New Matrix to a Sample File” in
Chapter 4 of the GeneScan Analysis Software User’s Manual.
3
If the Analysis Control window is not visible, choose Analysis Control from the
Windows pull-down menu.
4
Assign a size standard to all sample files as described in “Define and Select the
Size Standard” on page 3-4.
5
Highlight the appropriate dye colors for each sample.
3-2 General Analysis and Evaluation Techniques
To analyze sample files:
Step
6
(continued)
Action
Define analysis parameters:
a.
From the File menu, select New.
b.
Click Analysis Parameters. The Analysis Parameters dialog box appears.
c.
Set the appropriate analysis parameters for your application as described in
Chapter 4 of the GeneScan Analysis Software User’s Manual. Be sure to
exclude the primer peak from the analysis range.
7
Click Analyze.
8
After the analysis is complete, verify the peak assignments for the size standard in
all sample files using one of the methods described below.
continued on next page
General Analysis and Evaluation Techniques 3-3
Define and Select the
Size Standard
Step
Action
1
Select one of the sample files in the Analysis Control window.
2
If a size standard file already exists, proceed to step 8. Otherwise, continue to
step 3 and create a size standard file now.
3
Open the Size Standard pop-up menu for the highlighted sample, and select Define
New.
4
Define the size standard. See Chapter 5 for the sizes of the fragments in the size
standards. For detailed information on defining size standards, refer to Chapter 4 of
the GeneScan Analysis Software User’s Manual.
5
Close the window.
6
Click Save.
7
Name the size standard file, and click Save.
8
Open the Size Standard pop-up menu at the top of the Size Standard column, and
select the appropriate size standard.
A diamond in this column
indicates the size standard
will be applied to the
corresponding sample file
9
Size standard pop-up menu
The size standard must be selected for all the samples except matrix standard
samples. The size standard is selected if a diamond appears in the R (red) column
for a particular sample. To select or deselect the size standard, hold down the
command key and click in the appropriate square
continued on next page
3-4 General Analysis and Evaluation Techniques
Verify Size-Standard First Method
Peak Assignments
Step
1
Action
Highlight the sample files of interest and display the sizing curve by selecting Size
Curve from the Sample menu.
The R^2 value and the coefficients of the curve are provided. The R^2 value is a
measure of the accuracy of fit of the best-fit second order curve.
Note
You can only display the sizing curve for a sample if a valid sizing curve
exists for that sample.
2
Check whether all the defined size standard peaks fall on the sizing curve and note
peaks that lie off the curve.
Note
The 250-bp fragment in the GeneScan-350 and GeneScan-500 Internal
Lane Size Standards does not fall on the sizing curve.
3
If all of the size standard peaks did not lie on the sizing curve for any samples,
define a new size standard for those samples as described in the GeneScan
Analysis Software User’s Manual and reanalyze.
Second Method
Step
Action
1
Select Results Control from the Window menu ( R).
2
From the View menu, select Align By Size.
Note
3
If fragments are aligned by size, this option will not be available.
Examine the GeneScan size standard peaks in overlapping groups of 16 samples
(Quick Tile Off). Verify that the size standard peaks are superimposed, as shown
below.
General Analysis and Evaluation Techniques 3-5
Second Method
Step
4
(continued)
Action
In the Results display table, peaks in the size standard definition are marked with a
bullet as shown below.
Scroll through the tables to verify the size standard peak assignments and note
which samples (if any) have incorrect assignments.
5
Define a new size standard for those samples with incorrect peak assignments, as
described in the GeneScan Analysis Software User’s Manual.
3-6 General Analysis and Evaluation Techniques
Third Method
Step
Action
1
Highlight the sample files of interest. From the Sample window, select Sample Info
( I). The Sample File Information window appears.
2
Each dye is listed in the Analysis records. Select the Red dye as shown below.
Note
3
The sample must already be analyzed.
In the column marked Peak Totals, confirm that the Dye Std and the Sample contain
the same numbers of peaks.
General Analysis and Evaluation Techniques 3-7
Evaluating Data Quality
Good Data Looks Electropherogram peaks should be sharp, well-defined, and scaled above 150 relative
Like This fluorescent units (RFU) as shown in Figure 3-1. The peaks corresponding to different
color dyes need not be of equal intensity but the data for the less intense colors should
be clearly resolvable at higher magnification (Figure 3-2).
Figure 3-1 Example of data from the Fluorescent Genotyping Demonstration Kit B. Two
dinucleotide repeat loci are labeled with each dye, except for red, which is used for the size
standard.
Figure 3-2 Expanded view of the D12S83 locus from the same sample as Figure 3-1
continued on next page
3-8 General Analysis and Evaluation Techniques
Bad Data Looks An example of data where the sample was greatly overloaded is shown in Figure 3-3.
Like This Note that even the “pull-up” peaks (see page 3-11) are truncated.
pull-up peaks
Figure 3-3 Ridiculously overloaded sample
A more subtle example of overloading is shown in Figure 3-4 and Figure 3-5. The
off-scale peaks in the raw data in Figure 3-4 (note that the peaks are truncated at
8100 RFU) appear smaller in the analyzed data in Figure 3-5. The peaks are
broadened and blue “pull-up” peaks (see page 3-11) appear under the green peaks.
off-scale peaks
Figure 3-4 Raw data from an overloaded sample
pull-up peaks
Figure 3-5 Analyzed data from sample in Figure 3-4
General Analysis and Evaluation Techniques 3-9
Quantitating Nucleic Acids
Introduction You can determine the relative quantities of two 5´-end labeled fragments run on your
ABI PRISM 310 Genetic Analyzer by comparing the corresponding peak areas or peak
heights on a GeneScan electropherogram.
IMPORTANT
Do not use internally-labeled ([F]dNTP-labeled) fragments in your
quantitative experiments. Variations in the per-fragment number of labeled nucleotides and the
increased peak spreading with this method make relative quantitation unreliable.
How to Proceed To determine the relative number of molecules of two different-sized fragments, you
calculate the ratio of respective peak areas or heights. Always compare peak area to
peak area and peak height to peak height.
♦
If two fragments are similar in size, it is often better to compare peak heights,
especially if the peaks overlap slightly.
If the peaks are well defined, peak area and peak height will give similar results. If
the peaks are irregularly shaped, e.g., have shoulders, peak heights will often give
better results than peak areas.
♦
If two fragments are far apart in size, it is often better to compare peak areas
because large peaks tend to spread considerably more than small peaks.
Ensuring Precise Depending upon the value you set for the Minimum Peak Half Width and the
Relative smoothing option that you choose, the GeneScan software may interpret a noisy peak
Quantitation as multiple peaks. Thus, these parameters can influence the measurement of peak
area and peak height. Overestimating the number of peaks can be a particular
problem with the jagged peaks characteristic of noisy data. Either increase the
Minimum Peak Half Width or use a stronger smoothing option when analyzing noisy
data.
3-10 General Analysis and Evaluation Techniques
Evaluating Matrix Quality
Purpose of a Matrix While the most intense fluorescence emitted by an ABI PRISM™ dye will fall within a
small wavelength detection range, some fluorescence emission in the detection
ranges of the other dyes will always occur. The multicomponent matrix compensates
for this overlap by subtracting out, in each dye’s detection range, the portion of the
signal due to fluorescence from other dyes.
For directions on how to create a matrix file, see Appendix B.
Why the Matrix When you create a matrix, you must run each relevant dye matrix standard separately
Must Be Remade to determine the proportional amount of fluorescence that is emitted in all four
detection regions. Because the emission spectra of the dyes vary with the physical
environment (such as the pH or polymer type and concentration), the matrix must be
remade if run conditions change.
Factors Affecting Matrix Quality
♦ Aging reagents
♦
Buffer type and concentration
♦
Polymer type
♦
Denaturing vs. non-denaturing conditions
♦
Run temperature
Virtual Filter Set C
The emission maximum of 6-FAM, the recommended blue-displaying dye for this filter
set, is very close to the laser wavelength of 514.5 nm. Thus, the window for collected
blue light-intensity data is offset to longer wavelengths and does not contain the
emission maximum of 6-FAM. It is also very close to the detection region for the
green-displaying dye TET (see “Virtual Filter Set C” on page 4-9).
Matrix files made for Virtual Filter Set C are especially susceptible to minor changes in
run conditions. If you are using Virtual Filter Set C for GeneScan applications, watch
for evidence of matrix problems and remake the matrix as soon as problems appear.
How to Recognize A poor or incorrect matrix results in too much or too little subtraction of dye spectral
Matrix Problems overlap during data analysis. Each causes a recognizable electropherogram anomaly:
♦
Bleedthrough peaks, also called “pull-ups” (caused by too little subtraction)
♦
Elevated interpeak baseline (caused by too much subtraction)
Bleedthrough Peaks (or Pull-ups)
Bleedthrough peaks are small peaks of one color lying directly under a large peak of
another color even though there is no PCR product corresponding to the smaller peak.
(The large-peak signal is “pulling-up” peaks in other colors.) An example is shown in
Figure 3-6 on page 3-12.
General Analysis and Evaluation Techniques 3-11
pull-up peaks
Figure 3-6 Characteristic appearance of bleedthrough peaks
Bleedthrough can occur for two reasons:
♦
The matrix was made with the wrong dyes or filter set.
For a list of recommended dye/filter set combinations, see “Recommended
Dye/Virtual Filter Set Combinations” on page 4-6.
♦
The signal from the large peak is off-scale because of sample overloading. In the
example shown in Figure 3-6, the peak showing bleedthrough is actually off-scale
(Figure 3-7).
Figure 3-7 Raw data from the bleedthrough example shown in Figure 3-6
Keep peak heights between approximately 150 and 4000 RFU. If sample data is
off-scale, do one of the following:
♦
Rerun the samples using a shorter injection time.
♦
Dilute and rerun the samples.
3-12 General Analysis and Evaluation Techniques
Elevated Interpeak Baseline
Figure 3-8 shows a typical example of an elevated interpeak baseline:
Figure 3-8 Characteristic appearance of an elevated baseline caused by a bad or incorrect
matrix
In this example, the green baseline is elevated in the region between two large black
peaks (representing the yellow dye signal) because too much green signal is
subtracted from the yellow signal (see Figure 3-9 on page 3-14). The GeneScan
software uses these low data points to calculate the baseline for the green signal.
Therefore the original green baseline is elevated.
Note
If the baseline is sufficiently elevated, random fluctuations in the baseline can lie above
the Peak Amplitude Threshold and might be falsely interpreted as product peaks.
If you suspect that an elevated interpeak baseline is caused by matrix problems,
inspect the data before baselining. This can be done by reanalyzing the data with
baselining deselected in the Analysis Parameters dialog box. As shown in Figure 3-9,
low data points are apparent as troughs in one color beneath peaks in another.
General Analysis and Evaluation Techniques 3-13
Figure 3-9 The data of Figure 3-8 before baselining
What To Do If You If problems related to bleedthrough peaks or to an elevated interpeak baseline appear
Have Matrix consistently, you should remake the matrix. Apply the new matrix to the old sample
Problems data and reanalyze the data.
For directions on how to create a matrix file, see Appendix B.
3-14 General Analysis and Evaluation Techniques
ABI PRISM Dyes
4
4
Overview
In This Chapter This chapter describes the dyes used in GeneScan® fragment analysis applications. It
also provides background information on the following issues:
♦
How to choose dye/virtual filter set combinations
♦
What factors determine the relative signal intensities of ABI PRISM™ dyes
♦
Why matrix files depend on the run conditions
This chapter contains the following topics:
Topic
See Page
Available Dyes
4-2
Understanding Dye Spectra
4-3
Choosing Dye/Filter Set Combinations
4-5
Emission Spectra for Representative Dye/Virtual Filter Set
Combinations
4-8
ABI PRISM Dyes 4-1
Available Dyes
Introduction Applied Biosystems supplies ten fluorescent dyes for use on ABI PRISM instruments:
5-FAM, 6-FAM, R110, TET, JOE, R6G, HEX, NED, TAMRA, and ROX. Each emits a
continuous spectrum of light upon laser excitation.
During an electrophoresis run, the ABI PRISM® 310 Genetic Analyzer records the
fluorescence intensity as a function of time and wavelength from regions on a CCD
camera that correspond to different detection wavelength ranges. A multicomponent
matrix is applied to the fluorescence intensity data to correct for spectral overlap
between the dyes. After correction, the fluorescence intensities are color-coded and
displayed as peaks in the electropherogram.
Dye Chemical Forms ABI PRISM dyes are available in multiple chemical forms. Some forms are supplied
coupled to primers and others you can use to label your own custom primers. Each
form has distinct advantages and disadvantages depending upon the intended
application and your laboratory setup.
The following table summarizes the uses of and dyes available in each chemical form:
Chemical Form
Used For...
Available Dyes
NHS-esters
Post-synthesis 5´-end labeling
of oligonucleotides containing
a 5´ Aminolink 2
NEDa, TAMRA, ROX
Phosphoramidite
reagents
Preparing custom, 5´-end
labeled primers directly on any
Applied Biosystems DNA
synthesizerb
6-FAM, HEX, TET,
NEDa
[F]dNTPs
Simple internal fluorescent
labeling of multiple nucleotides
during PCR amplification
R6G, R110, TAMRA
Labeled primers in
reagent kits
Microsatellite and human
identification applications
5-FAMc, JOEc,
6-FAM, HEX, TET,
NEDa
Labeled size
standard
Generating the sizing curve
to size unknown sample
fragments
TAMRA, ROX
a. NED-labeled primers are available only in kits or through the Applied Biosystems
Custom Oligo Service. Call Applied Biosystemsor visit the Applied Biosystems
WorldWideWeb page at www.appliedbiosystems.com/techsupport for information on how
to order custom-labeled oligos.
b. For directions on synthesizing labeled oligonucleotides, see Appendix C.
c. 5-FAM and JOE are only available as labeled primers in select reagent kits.
See “Choosing Fluorescent Labeling Methods” on page 2-5 for a detailed comparison
of fluorescent labeling with 5´-end labeled primers and [F]dNTPs.
4-2 ABI PRISM Dyes
Understanding Dye Spectra
Background An electron, in a molecule or atom, that has been transferred to an excited (high
energy) state, e.g., after absorption of a photon, will eventually return to the more
stable (lower energy) ground state. The return to the ground state can occur either
through the evolution of heat (radiationless decay) or through the emission of a photon
(fluorescence or phosphorescence).
Definitions The emission spectrum of a fluorescent dye is the intensity of emitted light
(fluorescence) as a function of the wavelength of the emitted light.
The excitation spectrum of a dye is the intensity of emitted light as a function of the
wavelength of the exciting light.
The excitation efficiency of a dye is a measure of the probability that it will absorb light
of a certain wavelength, as a percentage of the probability of absorption at the
wavelength of maximum absorption.
The quantum yield of a dye is the probability that its excited state will emit a photon as
it decays back to the ground state.
Factors That Affect The emission and excitation spectra of a dye attached to DNA depend upon the dye’s:
Spectra ♦ Chemical structure
♦
Physical environment
Relevant parameters include the buffer pH and concentration, the polymer
composition, and whether the DNA is single- or double-stranded.
The effect of the physical environment on dye spectra explains why you need to
remake the matrix every time you change the run conditions.
Although altered by the physical environment, the wavelengths of maximum emission
and excitation for each ABI PRISM dye always lie within a small wavelength range. This
relative invariance of the emission spectra is crucial to experimental success.
Experimental Detecting a Dye Signal
Considerations The ability of the instrument to detect a dye signal depends upon the dye’s:
♦
Excitation efficiency at the wavelengths of light emitted by the laser
The argon ion laser in the ABI PRISM 310 Genetic Analyzer emits the greatest
intensity of light at 488 nm and 514.5 nm.
♦
Quantum yield
♦
Concentration
Distinguishing Between Two Dye Signals
The instrument identifies a dye by determining the ratio of the dye’s emission
intensities in a series of filters. Each dye’s maximum emission intensity lies in a unique
filter.
The ability of any instrument to distinguish between two dye signals is determined by
the relative differences in the measurements of the two dyes in each of two filters. The
ABI PRISM Dyes 4-3
larger the difference in the intensity of the signal in the two filters, the easier it is to
identify each dye. The closeness of the ratios of the measurements in each of the
filters will be determined by the amount of overlap in the two emission spectra.
In general, the ability to discern between two dye signals is enhanced by:
ABI PRISM Dye
Maximum Emission
and Excitation
Wavelengths
♦
A larger separation between the emission maxima of the two dyes
♦
A narrower emission spectrum of one or both dyes
The following table lists the maximum fluorescence emission and excitation
wavelengths for oligonucleotides labeled with ABI PRISM dye NHS-esters, dye
phosphoramidites, and [F]dNTPs. (The actual maximum emission and excitation
wavelengths may differ from the listed values due to the influence of the physical
environment upon the dye.)
Table 4-1 Maximum Emission and Excitation Wavelengths
Emission λmax
(nm)
Excitation λmax
(nm)
6-FAM
517
494
5-FAM
522
493
R110
525
501
TET
538
522
Dyea
R6G
549
529
HEX
553
535
JOE
554
528
TAMRA ([F]dNTP)
572
555
NED
575
553
TAMRA
583
560
ROX
607
587
a. All dye-labeled oligonucleotides were run at 10-7 M in 1X TE buffer, pH 8.0, room
temperature, on a TaqMan® LS-50B PCR Detection System.
4-4 ABI PRISM Dyes
Choosing Dye/Filter Set Combinations
How Data Collection The ABI PRISM 310 Genetic Analyzer determines the light intensity in four
Works non-overlapping regions on a CCD camera. Each region corresponds to a wavelength
range that contains or is close to the emission maximum of an ABI PRISM dye. The
exact positions of the regions and the dye combinations appropriate to these positions
depend upon the virtual filter set used.1 For example, with Virtual Filter Set A the
instrument records the light intensity in four regions, or “windows,” centered at 540 nm,
560 nm, 580 nm, and 610 nm. The window positions in each virtual filter set have
been optimized to provide the maximum possible separation among the centers of
detection for the different dyes while maintaining an excellent signal-to-noise ratio.
The GeneScan Analysis Software color-codes the intensity displays from the four
light-collection regions. These appear as the blue, green, black, and red peaks in the
Raw Data window. The blue display represents the total light intensity from the
shortest wavelength range monitored and the red display represents the total light
intensity from the longest wavelength range monitored.
It is important to realize that the same four colors are used to color-code fluorescence
data from all dye/virtual filter set combinations. Thus, the display colors represent the
relative, not the actual, detection wavelengths.
The process is similar to using physical filters to separate light of different
wavelengths. However, the ABI PRISM 310 Genetic Analyzer filter sets are called
“virtual filters” because the instrument uses no physical filtering hardware to perform
the separation.2
Available Virtual The ABI Prism 310 Genetic Analyzer uses six virtual filter sets, A–F.
Filter Sets
Virtual filter sets A, C, D, and F are used for GeneScan applications, while A, B, and E
are used for DNA sequencing applications.
Note
You can change the virtual filter set used for one or more injections in a series of
capillary injections by selecting a different run module in the GeneScan Injection List.
Rules for Dye Choice Each filter set should be used with a combination of four or fewer dyes (including the
dye reserved for the internal lane size standard) that:
♦
Display in four different colors
♦
Are available in compatible chemical forms
You can combine phosphoramidite labels with NHS-ester labels. You should not
combine [F]dNTP-labeling with any other labeling method.
Table 4-2 through Table 4-4 on pages 4-6 and 4-7 will help you chose the appropriate
dye and filter set combination for your particular application.
1.
Each GeneScan run module contains instructions for a specific virtual filter set. Once you choose a
module, the choice of virtual filter set is automatic.
2.
The ABI PRISM 310 Genetic Analyzer has a long-pass filter to prevent light from the instrument’s argon
ion laser from interfering with the detection of the dye signals.
ABI PRISM Dyes 4-5
Table 4-2 Chemical Forms and Color Displays of ABI PRISM Dyes
Dye
Available As...
Color Display
(in Virtual Filter Set)
5-FAMa
Labeled primer in reagent kits
Blue (A, F)
6-FAM
Phosphoramidite
Blue (A, C, D)
R110
[F]dNTP
Blue (A)
TET
Phosphoramidite
Green (C)
JOEa
Labeled primer in reagent kits
Green (A, F)
R6G
[F]dNTP
Green (A)
HEX
Phosphoramidite
Green (A, D), Yellow (C)
NEDb
NHS-ester, phosphoramidite
Yellow (D, F)
TAMRA
NHS-ester, [F]dNTP, or GeneScan Internal
Lane Size Standard
Yellow (A), Red (C)
ROX
NHS-ester or GeneScan Internal Lane Size
Standard
Red (A, D, F)
a. 5-FAM and JOE are only available as labeled primers in certain reagent kits (see Table 4-4 on page 4-7).
b. NED-labeled primers are available only in kits or through the Applied Biosystems Custom Oligo Service.
Call Applied Biosystems or visit the Applied Biosystems WorldWideWeb site at
www.appliedbiosystems.com/techsupport for information on how to order custom-labeled oligos.
Table 4-3 Recommended Dye/Virtual Filter Set Combinations
Chemical Forms
Combined
Use with Virtual
Filter Set...
6-FAM, HEX, TAMRA, ROX (std)
Phosphoramidites,
NHS-esters
A
R110, R6G, TAMRA, ROX (std)
[F]dNTPs
5-FAM, JOE, TAMRA, ROX (std)
Reagent kit primers,
NHS-esters
6-FAM, TET, HEX, TAMRA (std)a
Phosphoramidites
C
6-FAM, HEX, NED, ROX (std)
Phosphoramidites
D
5-FAM, JOE, NED, ROX (std)
Reagent kit primers,
NHS-esters
F
Dye Combination
a. This combination, although recommended, can sometimes give poor quality data due to spectral overlap
among the dye signals. If you experience matrix problems with this combination, you may see an
improvement in data quality by switching to 6-FAM, HEX, NED, and ROX and using Virtual Filter Set D.
4-6 ABI PRISM Dyes
Table 4-4 Reagent Kit and Custom-labeled Primer Dye Sets
Virtual
Filter Set
Application
Dye Set
AmpFl STR Blue™ PCR Amplification Kit
5-FAM (Blue), ROX (Red, std)
A, F
JOE (Green), ROX (Red, std)
A, F
StockMarks® for Horses Equine Paternity
PCR Typing Kit
5-FAM (Blue), JOE (Green),
TAMRA (Yellow), ROX (Red,
std)
A
ABI PRISM™ Linkage Mapping Set
6-FAM (Blue), TET (Green),
HEX (Yellow), TAMRA (Red,
std)
C
StockMarks for Cattle® Bovine Paternity
PCR Typing Kit
Custom-labeled primers for fragment
analysis
6-FAM (Blue), HEX (Green),
NED (Yellow), ROX (Red, std)
D
5-FAM (Blue), JOE (Green),
NED (Yellow), ROX (Red, std)
F
AmpFl STR
Kit
Green™
I PCR Amplification
ABI PRISM Linkage Mapping Set
Version 2
AFLP™ Microbial Fingerprinting Kit
AFLP Plant Mapping Kits
AmpFl STR™ Profiler™ PCR Amplification
Kit
AmpFl STR Profiler Plus™ PCR
Amplification Kit
ABI PRISM Dyes 4-7
Emission Spectra for Representative Dye/Virtual Filter Set Combinations
About the Spectra In the following four figures, the collection windows of the four GeneScan virtual filter
sets are shown overlaid with the normalized emission spectra of a recommended dye
set.
The wavelength of maximum emission of the dyes shown in these figures differs from
the value given in Table 4-1 on page 4-4 for the following reasons:
♦
The long-pass blocking filter (see footnote on page 4-5) blocks much of the light
emitted by 6-FAM and 5-FAM, the dyes with emission maxima closest to the laser
wavelength.
♦
The environment of the capillary polymer shifts the emission spectra of ABI PRISM
dyes.
See “Factors That Affect Spectra” on page 4-3 for an explanation of the observed
shift.
Virtual Filter Set A Virtual Filter Set A is used with the dyes in the Dye Primer Matrix Standards Kit
NORMALIZED FLUORESCENCE INTENSITY
(5-FAM, JOE, TAMRA, and ROX).
continued on next page
4-8 ABI PRISM Dyes
Virtual Filter Set C The following figure demonstrates why matrix problems can occur using this virtual
NORMALIZED FLUORESCENCE INTENSITY
filter set. The light collection windows for 6-FAM and TET are close to one another and
the spectral overlap between the two dyes is significant.
Virtual Filter Set D The spectral resolution of this dye/virtual filter set combination is much greater than
the spectral resolution of 6-FAM, TET, HEX, and TAMRA with Virtual Filter Set C.
Switching to this combination reduces the potential for matrix problems and may yield
cleaner data.
continued on next page
ABI PRISM Dyes 4-9
Virtual Filter Set F The spectral resolution of this dye/virtual filter set combination is similar to the spectral
resolution of 5-FAM, JOE, TAMRA, and ROX with Virtual Filter Set A. However, if you
are experiencing problems with signal strength using TAMRA or you want to load less
sample, you should use this combination. (Relative signal strength is not indicated in
these normalized spectra.)
NORMALIZED FLUORESCENCE INTENSITY
Virtual Filter Set F is used in the AmpFl STR Profiler and AmpFl STR Profiler Plus
PCR Amplification Kits and in the AFLP Plant Mapping and AFLP Microbial
Fingerprinting Kits.
4-10 ABI PRISM Dyes
Sizing and Size
Standards
5
5
Overview
In This Chapter This chapter describes the size-calling process in detail, including the following:
♦
The distinction between absolute accuracy and precision in size calling
♦
How cross-platform sizing differences arise
♦
How to avoid or recognize the most common sizing problems
This chapter also describes the available GeneScan Internal Lane Size Standards,
including each standard’s useful range.
This chapter contains the following topics:
Topic
See Page
Introduction to Sizing
5-2
Preventing/Troubleshooting Sizing Problems
5-5
GeneScan Internal Lane Size Standards
5-7
GeneScan-350 Size Standard
5-8
GeneScan-400HD Size Standard
5-10
GeneScan-500 Size Standard
5-12
GeneScan-1000 Size Standard
5-14
GeneScan-2500 Size Standard
5-16
Sizing and Size Standards 5-1
Introduction to Sizing
Introduction Size standards and sample fragments loaded in the same capillary run undergo the
same electrophoretic forces. Therefore, the relative electrophoretic mobility of any
sample fragment is a good indicator of its molecular weight because of
injection-to-injection variation in electrophoretic forces no longer contributes to
measurement error.
Process Overview The three steps in the size-calling process are the following:
Fitting the Internal Lane Size Standard to the Size Standard Definition
During this first step, the GeneScan® Analysis Software tries to match the peaks of
the internal lane standard with the peaks of the size standard definition, so that the
overall fit:
♦
Maximizes the number of matched peaks
To be considered a match, a size standard peak must lie within ±400 scans of its
expected position (as defined by the corresponding size standard definition peak).
♦
Minimizes the total squared error of the matched peaks
Once a size standard peak is matched, the “error” is defined as the distance
between its expected position and its actual position in the internal lane standard.
To complete Step 1 successfully, the GeneScan Analysis Software must match at
least three peaks.
Generating a Sizing Curve
From the fragment migration times of the internal lane standard, the GeneScan
Analysis Software generates a sizing curve giving size in base pairs or nucleotides as
a function of scan number (i.e., migration time) using one of the following
operator-chosen sizing methods:
♦
♦
Global sizing methods
–
2nd-Order Least Squares
–
3rd-Order Least Squares
–
Global Southern
Local sizing methods
–
Local Southern
–
Cubic Spline
Global methods, which generate the best-fit curve from all matched fragments in the
size standard, are less affected than local methods by anomalies in the run times of
single size standard fragments.
Local methods, which generate the best-fit curve from nearby internal lane standard
data points, are less affected by changes in the electrophoresis conditions or in the
analysis range. (A change in the analysis range will change the subset of size
standard fragments that is available for generating the sizing curve.)
IMPORTANT
For the Local Southern Method to work, you must have at least two size
standard fragments larger than your largest unknown fragment.
5-2 Sizing and Size Standards
For detailed information on the different sizing methods, refer to the GeneScan
Analysis Software User’s Manual.
Converting Fragment Migration Times to Sizes
This step is a straightforward mapping of any given fragment’s migration time onto the
sizing curve.
Accuracy Versus Accuracy in size calling is a measure of the instrument’s ability to generate fragment
Precision sizes that are close to the actual size of the fragment as determined by sequencing.
Precision, or reproducibility, in size calling is a measure of the instrument’s ability to
generate the same size consistently for a given fragment independent of whether the
called size is close to the actual size for a given set of run conditions.
Comparing Sizes
Obtained
Within and Across
Platforms
If care is taken to control for variations in run conditions, ABI PRISM® instruments are
highly precise within a single set of injections or a single gel. However, the called size
for the same fragment can differ between run conditions on a single instrument. In
other words, the generated sizes are not necessarily accurate.
Between-run sizing differences arise from a number of factors including:
♦
Differences in the type and concentration of capillary or gel polymer
♦
Well-to-read or time-to-read differences
♦
Differences in run temperature
♦
Differences in electrophoresis conditions (e.g., the denaturing ability of the
separation matrix)
♦
Changes in the sizing method or specific GeneScan size standard used to
generate the sizing curve
When comparing across injections, it is important to use the same sizing method
and the same size standard definition.
Table 5-1 on page 5-4 compares precision within and between the three instrument
platforms for a typical data set from the AmpFl STR Blue™ PCR Amplification Kit. The
three instrument platforms represented are the following:
♦
ABI PRISM® 377 DNA Sequencer, 36-cm wtr plates
♦
ABI™ 373 DNA Sequencer, 24-cm wtr plates
♦
ABI PRISM 310 Genetic Analyzer, POP-4™ polymer
Sizing and Size Standards 5-3
All results were obtained within a gel or within a set of injections from a single
capillary.
Table 5-1 Cross-platform precision results obtained from the AmpFl STR Blue PCR
Amplification Kit
ABI PRISM 377
Allele
ABI 373
ABI PRISM 310
n
Actual Size
Mean
S. D.
Mean
S.D.
Mean
S.D.
12
3
114
114.23
0.05
114.53
0.15
111.89
0.07
19
3
142
143.36
0.08
143.06
0.04
140.55
0.01
11
3
157
157.25
0.06
157.62
0.03
155.20
0.01
21
3
197
196.98
0.03
197.16
0.05
195.50
0.06
18
4
219
220.25
0.05
217.73
0.11
217.15
0.05
30
18
267
268.87
0.05
265.20
0.13
265.68
0.10
D3S1358
vWA
FGA
For example, consider D3S1358 allele 12. On all three platforms, three times the
standard deviation is less than 0.5 bp. By contrast, the mean called size for this allele
differs by more than 2 bp between the ABI PRISM 310 and ABI PRISM 377 instruments.
IMPORTANT
Because the called size for a fragment can differ from its actual size, you
should convert fragment sizes to alleles before comparing microsatellite data generated on
different instruments.
5-4 Sizing and Size Standards
Preventing/Troubleshooting Sizing Problems
Preventing Sizing The following guidelines will help you avoid some of the more common sources of
Problems inconsistent sizing within a single experiment:
Guidelines
Comments
Use the same sizing method for all
injections.
To verify, check the Analysis Record in the
Sample Information window.
Define the same size standard peaks in the
size standard definition for all injections (if
using more than one size standard
definition).
To verify, overlay the size standard peaks
from each injection or display the sizing
curve for each sample file.
Verify that all defined size standard peaks
are called within all sample files.
In the Analysis Record in the Sample
Information window, make sure that
Standard Defined and Standard Matched
are the same.
Use the same Analysis Range in the size
standard definition and in the sample files to
be analyzed.
To verify, check defined data points in the
Analysis Parameters window.
What Can Go If the position of a size standard peak differs by more than ±400 scans from the
Wrong definition peak, the GeneScan Analysis Software will not recognize the peak.
The most common causes of failure to recognize a size standard peak are the
following:
♦
Bad capillaries
♦
Bleedthrough peaks caused by:
–
Matrix problems
–
Off-scale data (e.g., too much sample is loaded or the primer peak is not
removed from the analysis range)
♦
Using anomalous size standard peaks in the size standard definition
♦
Changes in electrophoresis conditions
Bad Capillaries
A bad capillary (e.g., one that is broken or has a dirty detection window) is the most
common cause of inconsistency in the scan position of size standard peaks. If you are
having sizing problems always double-check the condition of the capillary.
Signs of a bad capillary include:
♦
Loss of current
♦
Loss of resolution
♦
Low or no signal
See “Troubleshooting PCR Product Detection” on page 11-7 for more information.
Sizing and Size Standards 5-5
Matrix Problems
If the multicomponent matrix is not correct, sample peaks in other colors will often
bleed through to the size standard color, creating false peaks and disrupting sizing.
Off-Scale Data
Off-scale data can also be the source of peaks that bleed through to the size standard
color, even when the matrix is good. See “Determining Loading Concentrations for
Samples” on page 2-8 and “Optimizing Electrokinetic Injection Parameters” on
page 2-9 for suggestions on evaluating and modifying signal strength.
Even if you load the correct amount of sample, sometimes the 35-bp fragment of the
GeneScan-350 and GeneScan-500 size standards co-migrates with one of the primer
peaks. In most cases the unused primer runs as a number of clustered, off-scale
peaks. Because matrix files cannot correct for off-scale data, bleedthrough peaks
inevitably appear in other colors. If the GeneScan Analysis Software mistakes one of
the bleedthrough peaks for the 35-bp size standard peak, the size-calling curve will be
inaccurate over part or all of its range.
Using Anomalous Size Standard Peaks
Using the following fragment peaks in the size standard definition can also cause
sizing problems:
♦
The 250-bp fragment peak of the GeneScan-350 and the GeneScan-500 size
standards under denaturing conditions
♦
The 262- and 692-bp fragment peaks of the GeneScan-1000 size standard under
non-denaturing conditions
♦
The 508-bp fragment peak of the GeneScan-2500 size standard under
non-denaturing conditions
The apparent size of these fragments is always smaller than their actual size. (For
example, the 250-bp fragment frequently runs at 246 bp.) The reason that they should
not be used is that their apparent size varies greatly with small changes in
experimental conditions. Using any of these fragment peaks in the size standard
definition will affect sizing precision.
Changes in Electrophoresis Conditions
All changes in electrophoresis parameters, buffers, and polymer composition affect
the fragment migration rate and can therefore affect sizing.
For More For more information on techniques for improving sizing accuracy on the
Information ABI PRISM 310 Genetic Analyzer, refer to Rosenblum et al. (1997) and Wenz et al.,
1998.
5-6 Sizing and Size Standards
GeneScan Internal Lane Size Standards
\
Definition Internal lane size standards are fluorescently-labeled DNA ladders that you load in the
same capillary injection as your experimental samples. The size standard fragments
are subject to the same electrophoretic forces as the experimental samples and
compensate for injection-to-injection variation in these forces. The uniform spacing of
size standard fragments ensures precise size calling throughout the size-calling
range.
Available Standards Applied Biosystems provides five different size standards labeled with either TAMRA
or ROX:
♦
GeneScan-350
♦
GeneScan-400HD
♦
GeneScan-500
♦
GeneScan-1000 (only available labeled with ROX)
♦
GeneScan-2500
IMPORTANT
Choose a size standard such that there at least two size standard fragments
larger than your largest unknown fragment.
Sizing and Size Standards 5-7
GeneScan-350 Size Standard
Useful Range You can use the GeneScan-350 size standard to determine fragment lengths between
35 and 350 base pairs.
Fragment Lengths The following table lists the lengths of the 12 fragments comprising the GeneScan-350
size standard:
Table 5-2 GeneScan-350: Fragment Lengths (nt)
35
139
250a
50
150
300
75
160
340
100
200
350
a. Do not use this fragment for sizing. See IMPORTANT notice on
page 5-9 for an explanation.
Preparation The GeneScan-350 size standard is prepared by digesting a proprietary DNA plasmid
with Pst I, followed by ligating a TAMRA- or ROX-labeled, 22-mer
oligodeoxynucleotide to the cut ends. A subsequent enzymatic digestion with BstU I
yields DNA fragments containing a single TAMRA or ROX dye.
continued on next page
5-8 Sizing and Size Standards
Denaturing Although the GeneScan-350 size standard is made of double-stranded DNA
Electropherogram fragments, only one of the strands is labeled. Consequently, even if the two strands
350
340
300
200
150
160
139
100
*
50
35
75
migrate at different rates under denaturing conditions you will not need to worry about
peak splitting. Figure 5-1 shows the peak patterns of GeneScan-350 fragments run
under denaturing conditions.
Figure 5-1 Electropherogram of the GeneScan-350 size standard run under denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using the POP-4
polymer at 60 °C.
IMPORTANT
An * for the 250-bp peak denotes a peak resulting from abnormal migration of
double strands that did not completely separate under denaturing conditions. Do not use this
peak to size samples. This peak shows variably smaller values than the actual size of the
fragments.
340
350
300
200
250
139
150
160
*
35
75
50
100
Non-denaturing Figure 5-2 shows the peak patterns of GeneScan-350 fragments run under
Electropherogram non-denaturing conditions.
Figure 5-2 Electropherogram of the GeneScan-350 size standard run under non-denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using 3% GeneScan
Polymer at 30 °C.
Sizing and Size Standards 5-9
GeneScan-400HD Size Standard
Useful Range You can use the GeneScan-400HD (High Density) size standard to determine
fragment lengths between 50 and 400 base pairs.
Special Uses The high density of marker bands in this standard makes it particularly useful for
microsatellite analysis. All fragments have been checked for migration that is true to
size under a wide variety of run conditions on all ABI PRISM instruments. There are no
anomalous fragments (e.g., the 250-bp fragment in GeneScan-350 on the
ABI PRISM 310 Genetic Analyzer).
Note
GeneScan-400HD is the recommended size standard for use with the ABI PRISM
Linkage Mapping Set Version 2.
Fragment Lengths The following table lists the lengths of the 21 fragments comprising the
GeneScan-400HD size standard:
Table 5-3 GeneScan-400HD: Fragment Lengths (nt)
50
160
260
360
60
180
280
380
400
90
190
290
100
200
300
120
220
320
150
240
340
Preparation All aspects of the preparation of the GeneScan-400HD size standard are proprietary.
Each fragment contains a single TAMRA or ROX fluorophore.
continued on next page
5-10 Sizing and Size Standards
Denaturing Although the GeneScan-400HD size standard is made of double-stranded DNA
Electropherogram fragments, only one of the strands is labeled. Consequently, even if the two strands
400
380
360
340
320
300
280
290
260
240
220
180
190
150
160
120
200
60
90
100
50
migrate at different rates under denaturing conditions you will not need to worry about
peak splitting. Figure 5-3 shows the peak patterns of GeneScan-400HD fragments
run under denaturing conditions.
Figure 5-3 Electropherogram of the GeneScan-400HD size standard run under denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using the POP-4
polymer at 60 °C.
400
380
360
340
320
280
290
300
240
260
200
220
180
190
120
150
160
60
90
100
50
Non-denaturing Figure 5-4 shows the peak patterns of GeneScan-400HD fragments run under
Electropherogram non-denaturing conditions.
Figure 5-4 Electropherogram of the GeneScan-400HD size standard run under
non-denaturing conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using
3% GeneScan Polymer (GSP) at 30 °C.
Sizing and Size Standards 5-11
GeneScan-500 Size Standard
Useful Range You can use the GeneScan-500 size standard to determine fragment lengths between
35 and 500 base pairs.
Special Uses These size standards are recommended for analysis of tri- and tetranucleotide
microsatellite loci, which can often exceed 400 base pairs in length.
.
Fragment Lengths The following table lists the lengths of the 16 fragments comprising the GeneScan-500
size standard:
Table 5-4 GeneScan-500: Fragment Lengths (nt)
35
139
250a
400
50
150
300
450
75
160
340
490
100
200
350
500
a. Do not use this fragment for sizing. See IMPORTANT notice on
page 5-13 for an explanation.
Preparation The GeneScan-500 size standard is prepared by digesting a proprietary DNA plasmid
with Pst I, followed by ligating a TAMRA- or ROX-labeled, 22-mer
oligodeoxynucleotide to the cut ends. A subsequent enzymatic digestion with BstU I
yields DNA fragments containing a single TAMRA or ROX dye.
continued on next page
5-12 Sizing and Size Standards
Denaturing Although the GeneScan-500 size standard is made of double-stranded DNA
Electropherogram fragments, only one of the strands is labeled. Consequently, even if the two strands
migrate at different rates under denaturing conditions you will not need to worry about
peak splitting.
490
500
450
400
340
350
*
300
200
139
150
160
100
75
35
50
Figure 5-5 shows the peak patterns of GeneScan-500 fragments run under
denaturing conditions.
Figure 5-5 Electropherogram of the GeneScan-500 size standard run under denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using the POP-4
polymer at 60 °C.
IMPORTANT
An * for the 250-bp peak denotes a peak resulting from abnormal migration of
double strands that did not completely separate under denaturing conditions. Do not use this
peak to size samples. This peak shows variably smaller values than the actual size of the
fragments.
490
500
450
400
340
350
300
250
200
139
150
160
35
75
50
100
Non-denaturing Figure 5-6 shows the peak patterns of GeneScan-500 fragments run under
Electropherogram non-denaturing conditions.
Figure 5-6 Electropherogram of the GeneScan-500 run under non-denaturing conditions on
the ABI PRISM 310 Genetic Analyzer. Fragments were run using 3% GeneScan Polymer (GSP)
at 30 °C.
Sizing and Size Standards 5-13
GeneScan-1000 Size Standard
Useful Range Under non-denaturing conditions, you can use the GeneScan-1000 size standard to
determine fragment lengths between 100 and 900 base pairs. Under denaturing
conditions using the POP-4 polymer, you can determine fragment lengths between
100 and 539 base pairs, the linear range (with respect to length in bp versus scan
number) of the separation.
Special Uses The GeneScan-1000 size standard fragments are labeled on both strands and thus
are most suited for non-denaturing applications. If run under denaturing conditions,
some or all of the peaks will appear split, making interpretation difficult. (Under
denaturing conditions, all fragments will run 18 nucleotides smaller than the sizes
shown in Table 5-5.)
Fragment Lengths The following table lists the lengths of the 17 fragments comprising the
GeneScan-1000 size standard.
Table 5-5 GeneScan-1000: Non-denatured Fragment Lengths (bp)
47
93
292
695
51
99
317
946
55
126
439
82
136
557
85
262a
692a
a. Do not use these fragments for sizing. See IMPORTANT notice on page 5-15 for an
explanation.
Note
Non-denatured fragments are 18 nucleotides longer than denatured fragments.
Preparation The GeneScan-1000 size standard is prepared by digesting pBR322 with the
restriction enzyme Alu I, followed by ligating a ROX-labeled, 22-mer
oligodeoxynucleotide to the cut ends.
continued on next page
5-14 Sizing and Size Standards
539
275
421
299
244
118
108
37
29
33
64
75
81
Denaturing Figure 5-7 shows the peak patterns of GeneScan-1000 fragments run under
Electropherogram denaturing conditions.
Figure 5-7 Electropherogram of the GeneScan-1000 size standard run under denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using the POP-4
polymer at 60 °C.
Note
Under denaturing conditions the two strands of the doubly-labeled GeneScan-1000
size standard fragments migrate at different rates, appearing as split peaks. To ensure
size-calling precision and a reliable size standard definition, you must explicitly define one peak
from each split peak pair in the size standard definition. To improve matching of size standard
peaks, choose either LeftMost Peak or RightMost Peak in the Split Peak Correction section of
the Analysis Parameters window.
*
946
695
557
439
*
126
85 82
93
99
55
136
317
293
Non-denaturing Figure 5-8 shows the peak patterns of GeneScan-1000 fragments run under
Electropherogram non-denaturing conditions.
Figure 5-8 Electropherogram of the GeneScan-1000 size standard run under non-denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using 3% GeneScan
Polymer (GSP) at 30 °C.
IMPORTANT
The * for the 262- and 692-bp peaks denote peaks resulting from abnormal
migration. Do not use these peaks to size samples. These peaks show variably smaller values
than the actual size of the fragments.
Sizing and Size Standards 5-15
GeneScan-2500 Size Standard
Useful Range Under non-denaturing conditions, you can use the GeneScan-2500 size standard to
determine fragment lengths between 100 and 5000 base pairs. Under denaturing
conditions using the POP-4 polymer, you can determine fragment lengths between
100 and 536 base pairs, the linear range (with respect to length in bp versus scan
number) of the separation.
Special Uses The GeneScan-2500 size standard fragments are labeled on both strands and thus
are most suited for non-denaturing applications. If run under denaturing conditions,
some or all of the peaks will appear split, making interpretation difficult. (Under
denaturing conditions, all fragments will run 18 nucleotides smaller that the sizes
shown in Table 5-6.)
Fragment Lengths The following table lists the lengths of the 27 fragments comprising the
GeneScan-2500 size standard.
Table 5-6 GeneScan-2500: Non-denatured Fragment Lengths (bp)
55
240
488
1740
4547
112
251
508a
2026
4789
127
256
554
2180
5117
134
287
845
2483
14097
190
304
1133
2499
204
379
1199
2878
a. Do not use this fragment for sizing. See IMPORTANT notice on page 5-17 for an
explanation.
Note
Non-denatured fragments are 18 nucleotides longer than denatured fragments.
Preparation The GeneScan-2500 size standard is prepared by digesting phage λ DNA with Pst I,
followed by ligating a TAMRA- or ROX-labeled, 22-mer oligodeoxynucleotide.
continued on next page
5-16 Sizing and Size Standards
490
470
361
269
286
222
233
238
109
116
94
536
186
172
Denaturing Figure 5-9 shows the peak patterns of GeneScan-2500 fragments run under
Electropherogram denaturing conditions.
Figure 5-9 Electropherogram of the GeneScan-2500 size standard run under denaturing
conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using the POP-4
polymer at 60 °C.
Note
Under denaturing conditions the two strands of the doubly-labeled GeneScan-2500
size standard fragments migrate at different rates, appearing as split peaks. To ensure
size-calling precision and a reliable size standard definition, you must explicitly define one peak
from each split peak pair in the size standard definition. To improve matching of size standard
peaks, choose either LeftMost Peak or RightMost Peak in the Split Peak Correction section of
the Analysis Parameters window.
14097
4547
4789
5117
2499
2878
2026
1740
1199
845
1133
488
379
304
287
240
251
256
190
204
*
554
55
112
127
134
2180/2483
Non-denaturing Figure 5-10 shows the peak patterns of GeneScan-2500 fragments run under
Electropherogram non-denaturing conditions.
Figure 5-10 Electropherogram of the GeneScan-2500 size standard run under
non-denaturing conditions on the ABI PRISM 310 Genetic Analyzer. Fragments were run using
3% GeneScan Polymer (GSP) at 30 °C.
IMPORTANT
An * for the 508-bp peak denotes a peak resulting from abnormal migration.
Do not use this peak to size samples. The peak has a smaller value than actual size of the
fragment.
Sizing and Size Standards 5-17
Optimizing PCR
6
6
Overview
In This Chapter The success or failure of most GeneScan® fragment analysis experiments depends
upon the success or failure of the PCR amplification step.
This chapter presents strategies that you can employ to optimize polymerase chain
reaction (PCR) product yield in your experiments. Because no single set of PCR
conditions is optimal for all applications, consider the optimization strategies
discussed in this section as hints or tips for improving PCR product yield.
This chapter contains the following topics:
Topic
See Page
Choosing Reaction Volumes and Tube Types
6-2
Designing Custom Primers
6-3
Determining Reagent Concentrations
6-6
Choosing the Right Enzyme
6-8
Multiplexing PCR
6-10
Using RNA Templates
6-12
Preventing Competing Side Reactions—Hot Start PCR
6-13
Modifying Thermal Cycling Parameters
6-15
Avoiding Contamination
6-16
3´ A Nucleotide Addition
6-18
Stutter Products
6-21
Preparing PCR Products for Analysis
6-23
Optimizing PCR 6-1
Choosing Reaction Volumes and Tube Types
Reaction Volumes With Applied Biosystems PCR Instrument Systems, reaction volumes in the range of
25–100 µL are generally used. However, reactions with less than 25 µL have been
successful.
Tube Types The following table lists the type of reaction tube to use with each thermal cycler.
Thermal Cycler
Reaction Tube Type
Uses
DNA Thermal Cycler
(TC1)
GeneAmp® PCR
Reaction Tubes
Optimized for PCR amplification of
reaction volumes between 25 µL and
100 µL. Mineral oil required.
DNA Thermal Cycler 480
0.5-mL GeneAmp
Thin-walled Reaction
Tubes with domed or
flat capsa
Allows you to program shorter hold
times (45 seconds or more) at each
temperature in the PCR cycle. Mineral
oil required.
GeneAmp PCR
System 9600
0.2-mL MicroAmp®
Reaction Tubes
Optimized for fast PCR amplification
of reaction volumes between 25 µL
and 100 µL. Use without mineral oil.
0.5-mL GeneAmp
Thin-walled Reaction
Tubes with domed
caps
Optimized for fast PCR amplification
of 100-µL reaction volumes. 48-well
adapter required. Mineral oil overlay or
AmpliWax® PCR Gems required.
GeneAmp PCR
System 9700
0.2-mL MicroAmp
Reaction Tubes
Optimized for fast PCR amplification
of reaction volumes between 25 µL
and 100 µL. Use without mineral oil.
GeneAmp PCR
System 2400
0.2-mL MicroAmp
Reaction Tubes
Optimized for fast PCR amplification
of reaction volumes between 25 µL
and 100 µL. Use without mineral oil.
a. Can also be used with the DNA Thermal Cycler (TC1) using hold times of at least 60 seconds.
Using Small Although reaction tubes usually do not need to be sterilized or siliconized, autoclave
Amounts of tubes when dealing with small quantities (approximately 150–500 pg) of starting DNA
Template template.
Autoclaved PCR tubes can also be ordered from Applied Biosystems:
6-2 Optimizing PCR
♦
MicroAmp Autoclaved Reaction Tubes with Caps, P/N N801-0612 (for the
GeneAmp PCR Systems 9600, 9700, and 2400)
♦
GeneAmp Autoclaved Thin-walled Reaction Tubes (with domed caps),
P/N N801-0611 (for the DNA Thermal Cycler 480)
Designing Custom Primers
Definition A PCR primer pair consists of two oligonucleotides, typically 15–30 nucleotides long,
that hybridize to complementary strands of the DNA template and flank the region of
interest.
To Ensure Successful Choose primers with similar melting temperatures (Tm).
Amplification
Choose primers that maximize the stability and specificity of binding to the desired
template.
Note
For best results, evaluate potential primers with the aid of primer-design software, e.g.,
Primer Express™.
Melting Choosing primers with similar Tms makes it possible to find thermal cycling
Temperature parameters that are optimal for all members of a primer pair or pairs. Be aware that
the calculated Tm is only a guideline (based on base composition). The actual Tm is
also influenced by the concentration of Mg2+, K+, and cosolvents.
Maximizing Stability Binding stability is influenced by:
♦
Primer/template base composition
♦
Primer/template base order
♦
Primer or template secondary structure
Effects of Base Composition
G-C bonds contribute more to the stability (increased melting temperature) of
primer/template binding than do A-T bonds.
To ensure stable binding of primer and template while avoiding problems with the
internal secondary structure of primers or long stretches of any one base, choose
primers with a 40% to 60% G+C content. However, do not let this rule interfere with
primer choice based on Tm and primer-length considerations. Avoiding primer-dimers
and gapped-duplex structures is more important than actual percent G+C.
Effects of Base Order
Two primer/template complexes with identical G+C content will have different melting
temperatures because base order influences the overall stability. You can determine
the exact effect of base order on complex stability using Table 6-1 (adapted from
Salser, 1978).
Table 6-1
Base-Pairing Energies (kcal/dinucleotide pair)
3´ Nucleotide
5´ Nucleotide
A
C
G
T
A
–1.2
–2.1
–2.1
–1.8
Note
C
–2.1
–4.8
–3.0
–2.1
G
–2.1
–4.3
–4.8
–2.1
T
–1.8
–2.1
–2.1
–1.2
In the table, larger negative values represent more stable interactions.
Optimizing PCR 6-3
To illustrate the use of the table, consider the two sequences 3´–GAC–5´ and
3´–CGA–5´. The sequence 3´–GAC–5´ contained within a primer would contribute
–4.2 kcal to the binding energy (–2.1 kcal [3´–GA–5´] + –2.1 kcal [3´–AC–5´] =
–4.2 kcal). However, if the G and C are next to each other, as in 3´–CGA–5´, the
contribution increases to –6.4 kcal (–4.3 kcal [3´–CG–5´] + –2.1 kcal [3´–GA–5´] =
–6.4 kcal).
Note
Although a G-C dinucleotide at the 3´ end of the primer can stabilize the binding
complex when using thermostable enzymes such as AmpliTaq® DNA Polymerase, a 3´ G-C can
also lead to false priming if you do not optimize PCR conditions. (For justification of the claim
that a 3´ G-C can lead to false priming, see “Minimizing Binding to Secondary Sites” on
page 6-4.)
Effects of Primer 2° Structure
Strings of Gs and Cs can form internal, non-Watson-Crick basepairs (Sarocchi et al.,
1970) that disrupt stable primer binding. Although this anomalous behavior is difficult
to predict, a good general rule is to avoid runs of more than three consecutive Gs in
primers. (See the following Note for exceptions to this rule.)
Note
A short run of G’s at or near the 5´ end of a primer will not disrupt stable primer binding
because 5´ positioning does not lead to involvement in disruptive secondary structures (for
example, primer-dimer or duplex loops).
Similarly, self-complementarity can lead to the formation of hairpin structures that
disrupt stable primer binding. A stable hairpin can form with just four G-C basepairs in
the stem and three bases in the loop (Summer et al., 1985).
Effects of Template 2° Structure
Primers do not bind effectively to target sequences with known secondary structure.
For example, RNA sequences often have regions of looped secondary structure.
Maximizing Maximizing binding specificity requires minimizing primer binding to secondary sites in
Specificity the DNA and to other primers.
Minimizing Binding to Secondary Sites
Note
This section is most applicable if your starting template is genomic DNA. The
probability of binding to secondary sites is greatly diminished for low-complexity templates such
as plasmid DNA.
Ideally, the binding of the primer to the desired template is:
♦
Strongest at the 5´ end.
♦
More positive than -9.8 kcal/mole at the 3´ end.
This is equivalent to saying that the binding at the 3´ end is weaker than
-9.8 kcal/mole.
Polymerases only require the binding of the nucleotides at the 3´ end to begin
elongation. If the 3´ nucleotides bind strongly (perhaps because of a 3´ G-C) any
template sequences that are complementary to the 3´ end are amplified. In this case,
because the entire primer is not used to discriminate among target sequences,
specificity is lost.
Conversely, if binding is strongest at the 5´ end, the typical binding event on the
template DNA begins at the 5´ end. Polymerases, however, cannot begin elongation
6-4 Optimizing PCR
until the 3´ end binds. Therefore the entire primer is used to distinguish among target
sequences.
Self-complementarity can lead to the formation of hairpin structures that decrease
binding specificity (as well as disrupt binding stability as discussed earlier).
Nucleotides in the hairpin structure are not available for recognition of the target
sequence. The available nucleotides can be thought of as forming a “smaller,” and
therefore less specific, primer.
When performing a computer-assisted search to evaluate binding to secondary sites
in the target DNA, consider the potential for “gapped duplex” formation.1
Note
Binding to secondary sites can also involve the formation of stable non-Watson-Crick
base pairs (Topal and Fresco, 1976). Stable base-pairing is most likely to occur between G and
T, but A-C and G-A pairs can also be stable (Hunter, 1986). All software programs have difficulty
modeling these sorts of interactions.
Minimizing Binding to Other Primers
Complementarity between two primers, especially at the 3´ ends, can lead to the
formation of product artifacts arising from amplified primer-dimers and
primer-oligomers. Avoid primers with regions of complementarity between members
of a primer pair or pairs.
Post-Amplification Adding 5´ primer-extensions (that are not complementary to the template) can
Manipulation facilitate a variety of useful post-amplification manipulations of the PCR product
without adversely affecting yield. Examples include 5´ extensions that contain
restriction sites, universal primer binding sites, or promoter sequences.
1.
A gapped duplex can form when the primer and target are completely complementary except for a
single base (Miller, Kirchoff et al., 1987; Miller, Wlodawer et al., 1987).
Optimizing PCR 6-5
Determining Reagent Concentrations
Factors to Consider When preparing reaction mixtures, consider the following factors that can affect overall
yield of specific DNA target sequences:
♦
dNTP concentration
♦
Magnesium ion concentration
♦
Primer concentration
♦
Template concentration
♦
Enzyme concentration
dNTP Concentration In the standard GeneAmp PCR protocol, the concentration of each deoxynucleoside
triphosphate (dNTP) is 200 µM.
In most cases, lower dNTP concentrations do not significantly affect the yield of PCR
amplification product and will increase the fidelity. However, for efficient base
incorporation, keep the four dNTP concentrations balanced and above the estimated
Km of each dNTP (10–15 µM).
Some applications might require higher dNTP concentration (especially when dNTP
analogues are used). However, excess dNTPs decrease enzyme fidelity.
Magnesium Ion DNA polymerases require free magnesium ion in solution for activity. For most PCR
Concentration amplifications, you can relate product yield and specificity and enzyme fidelity to the
free magnesium ion (Mg2+) concentration:
[free Mg2+] = [total Mg2+] – [total dNTP] – 2[EDTA]
In general, increasing the free magnesium concentration increases yield and
decreases specificity and fidelity.
To identify the magnesium concentration that gives the best compromise between
yield and specificity or fidelity for your particular application, perform the following
experiment. In the presence of 800 µM total dNTP concentration, run a MgCl2 reaction
series in 50-µM increments over the range from 100–400 µM MgCl 2 and identify the
optimal concentration.
continued on next page
6-6 Optimizing PCR
Template The concentration of template in your sample can affect the success of PCR
Concentration amplification in a variety of ways. Too much template promotes nonspecific binding of
primers to secondary sites or changes the pH of the reaction mix. Too little template
can result in poor yields, especially if the template is degraded.
Even very low template concentrations (10 copies) are often sufficient for successful
PCR amplification.
If your starting sample is DNA, you can use up to 20,000 copies of the target to start
optimization trials. In general, this translates to:
♦
1–5 ng of cloned template
♦
200 ng to 1 µg of genomic DNA
Start optimization trials with less genomic DNA if starting material is limited. With
clean, good quality genomic DNA, 500–1000 pg of starting material almost always
works well.
Enzyme For most PCR applications, 2.0–2.5 units of AmpliTaq Gold™ DNA Polymerase is
Concentration recommended for each 100-µL reaction volume.
Note
You can avoid the tedium and inaccuracies involved in pipetting 0.5-µL amounts of
enzyme by adding the enzyme to a fresh Master Mix prepared for a number of reactions.
Optimizing PCR 6-7
Choosing the Right Enzyme
Introduction For most applications AmpliTaq Gold DNA Polymerase is the enzyme of choice.
However, Applied Biosystems supplies a number of PCR enzymes that have been
optimized for specific needs. For quick reference, an enzyme-choice table is included
at the end of this section.
PCR Enzyme A brief summary of the seven PCR enzymes supplied by Applied Biosystems follows.
Overview
Derivatives of Native Taq DNA Polymerase
♦ AmpliTaq DNA Polymerase
AmpliTaq DNA Polymerase is a recombinant form of Taq DNA Polymerase
obtained by expressing a modified Taq DNA Polymerase gene in an E. coli host.
Like native Taq DNA Polymerase, it lacks endonuclease and 3´-5´ exonuclease
(proofreading) activities, but has a 5´-3´ exonuclease activity.
♦
AmpliTaq Gold DNA Polymerase
AmpliTaq Gold DNA Polymerase is a chemically modified form of AmpliTaq DNA
Polymerase. It provides the benefits of Hot Start PCR (that is, higher specific
product yield, increased sensitivity, and success with multiplex PCR) without the
extra steps and modifications of experimental conditions that make Hot Start
impractical for high throughput applications. AmpliTaq Gold DNA Polymerase is
delivered in an inactive state. A prePCR heating step of 10–12 minutes at 95 °C,
which can be programmed into the thermal cycling profile, activates the enzyme.1
For low template copy number amplifications, step-wise activation of AmpliTaq
Gold DNA Polymerase, or Time Release PCR, can prove useful.2
♦
AmpliTaq DNA Polymerase, LD
AmpliTaq DNA Polymerase, LD (Low DNA), is the same enzyme as AmpliTaq
DNA Polymerase. However, the LD formulation has undergone a further
purification process. The purification step insures that false-positive PCR products
will be effectively minimized when amplifying bacterial sequences. AmpliTaq DNA
Polymerase, LD is especially useful for low-copy number amplifications.
♦
AmpliTaq DNA Polymerase, Stoeffel Fragment
AmpliTaq DNA Polymerase, Stoeffel Fragment, is a modified form of AmpliTaq
DNA Polymerase from which the N-terminal 289 amino acids have been deleted.
It is approximately twofold more thermostable than AmpliTaq DNA Polymerase
allowing higher denaturation temperatures for GC-rich templates or templates with
complex secondary structure. It lacks 5´-3´ exonuclease activity making it useful in
multiplex PCR. Finally, it is active and specific over a wide range of magnesium
ion concentrations (2 –10 mM).
6-8 Optimizing PCR
1.
A prePCR incubation heating step of 10 minutes at 95 °C activates approximately 40% of the enzyme
molecules. This is sufficient to perform efficient amplification during the early cycles when target copy
number is low. Because more enzyme is activated during each denaturation step, enzyme activity
increases as the number of target molecules increases, providing optimal PCR performance.
2.
In Time Release PCR, the prePCR heating step is omitted and the total number of cycles is increased.
Because the activation step is omitted, very little active enzyme is present during the first few PCR
cycles and many additional cycles are necessary for good results.
UlTma® DNA Polymerase
UlTma DNA Polymerase is obtained by expressing a modified form of the Thermotoga
maritima (Tma) DNA polymerase gene in an E. coli host. It lacks a 5´-3´ exonuclease
activity but retains a 3´-5´ exonuclease proofreading activity. It is recommended when
a high degree of fidelity is required.
Derivatives of Tth DNA Polymerase
Applied Biosystems supplies two modified forms of Thermus thermophilus (Tth) DNA
Polymerase:
♦
rTth DNA Polymerase
rTth DNA Polymerase is obtained by expression of a modified form of the Tth
gene in an E. coli host.
♦
rTth DNA Polymerase, XL
rTth DNA Polymerase, XL (Extra Long), provides the same features as rTth DNA
Polymerase for target sequences from 5–40 kb in length. An inherent 3´-5´
exonuclease activity allows for the correction of nucleotide misincorporations that
might otherwise terminate synthesis prematurely.)
Enzyme Choice If your application has special requirements, the table below will help you choose the
Table best enzyme:
Table 6-2 Application Requirements and Recommended Enzymes
If your application requires...
Use...
High specificity
AmpliTaq Gold DNA Polymerase
High sensitivity
AmpliTaq Gold DNA Polymerase
High fidelity
UlTma DNA Polymerase
High temperatures
AmpliTaq DNA Polymerase, Stoeffel
Fragment
UlTma DNA Polymerase
Multiplex PCR
AmpliTaq Gold DNA Polymerase
Amplification of low-copy number template
AmpliTaq Gold DNA Polymerase
AmpliTaq DNA Polymerase, LD (for bacterial
sequences)
High specificity at high ionic strength
AmpliTaq Gold DNA Polymerase
AmpliTaq DNA Polymerase, Stoeffel
Fragment
Amplification of extra-long fragments (>5 kb)
rTth DNA Polymerase, XL
PrePCR conversion to cDNA
rTth DNA Polymerase
Extra cycles
AmpliTaq DNA Polymerase, Stoeffel
Fragment
UlTma DNA Polymerase
High Mg2+ concentration
AmpliTaq Gold DNA Polymerase
AmpliTaq DNA Polymerase, Stoeffel
Fragment
Optimizing PCR 6-9
Multiplexing PCR
Definition Multiplex PCR is a technique for simultaneously amplifying multiple DNA targets using
multiple primer pairs in the same PCR reaction.
Advantages Multiplex PCR can:
♦
Simplify PCR setup
♦
Increase throughput
♦
Decrease cost per amplification
Limitations Potential limitations to multiplex PCR include:
♦
Primer-oligomer formation
♦
Loss of specificity
♦
Decreased yield of specific products
Overcoming these limitations can require a significant amount of optimization.
Enzyme Choice The high specificity of AmpliTaq Gold DNA Polymerase typically permits amplifying
with elevated Mg2+ concentrations for increased yield.
Primer Quality Because reactants (such as dNTPs) are often limiting during multiplex PCR, using
high quality primers is particularly important. For example, the decreased specificity
(and thus the increased reagent consumption) of one pair of degraded PCR primers
can prevent the success of the entire multiplex reaction. Although you can
compensate for a degraded pair of primers to some extent by increasing the
concentration of the other primer pairs, the increased cost per reaction and the
decreased reproducibility over time do not justify this short-term solution.
When buying or making primers make sure that they are length purified and that they
are free of contaminants.
Primer-Pair Typically, start out with equal concentrations for all primer pairs.
Concentrations
It will often be necessary to adjust the concentration of primer pairs in the multiplex
reaction until the peak heights are relatively even.
6-10 Optimizing PCR
♦
Increase the primer-pair concentration for fragments showing weak amplification.
♦
Decrease the primer-pair concentration for fragments showing significantly
greater than average amplification.
Troubleshooting Consider amplifying separately any primer pair that fails to amplify after its
Multiplex PCR concentration is increased.
To get rid of interfering background peaks, try:
♦
Swapping primer pairs between different multiplex reactions
♦
Removing primer pairs from the multiplex reaction
Optimizing PCR 6-11
Using RNA Templates
Suitable Templates RNA templates can be single- or double-stranded. If your starting sample is RNA,
then your template can be:
♦
Total cellular RNA
♦
Poly (A+) RNA
♦
Viral RNA
♦
tRNA
♦
rRNA
Two-Step RNA-PCR To synthesize first-strand cDNA prior to performing conventional PCR amplification,
you can use a reverse transcriptase such as MuLV or you can use rTth DNA
Polymerase.
In the presence of MnCl2, rTth DNA Polymerase will efficiently reverse transcribe RNA
to cDNA. After chelating the manganese ions with EGTA and adding MgCl2, rTth DNA
Polymerase can act as a thermostable DNA polymerase in a subsequent reaction in
the same tube.
Note
For RNA templates with a high GC content or complex secondary structure, Applied
Biosystems recommends using rTth DNA polymerase because of its high-temperature reverse
transcriptase activity and thermostable DNA polymerase activity.
Single-Step Using the GeneAmp EZ rTth RNA PCR Kit (P/N N808-0178), you can perform reverse
RNA-PCR transcription and PCR amplification in successive reactions in the same tube without
buffer changes or reagent additions. By combining programmed changes in
temperature with the action of Bicine, which is capable of buffering both metal and
hydrogen ions, in the EZ Buffer, the GeneAmp EZ rTth RNA PCR Kit enables you to
control a complex interaction of factors (metal ion concentration, pH, and ionic
strength) affecting enzyme activity.
Note
When amplifying multiple samples, making buffer changes is time-consuming and
increases the likelihood of contamination. The EZ Buffer affords full dUTP compatibility for
AmpErase® UNG-mediated carryover prevention.
For More Refer to the TaqMan® Gold RT-PCR Kit Protocol (P/N 402876) and the TaqMan EZ
Information RT-PCR Kit Protocol (P/N 402877) for more information.
6-12 Optimizing PCR
Preventing Competing Side Reactions—Hot Start PCR
When to Use Consider using the Hot Start technique whenever you need to improve the specificity
Hot Start and sensitivity of your PCR amplifications. Loss of specificity and sensitivity are often
caused by competing side reactions, which usually occur during the prePCR setup
period while all reactants sit together at permissive temperatures. (A common
competing side reaction involves the amplification of nontarget sequences in
background DNA either due to mispriming or to primer oligomerization.)
Limitations and The technique is cumbersome. If you have high throughput needs, switching to
Alternatives AmpliTaq Gold DNA Polymerase will give the same benefits as performing the Hot
Start technique, without the need for using wax barriers or opening reaction tubes. In
particular, if you are already using AmpliTaq Gold DNA Polymerase, performing the
Hot Start technique will not improve the specificity and sensitivity of PCR
amplification.
How Hot Start In the Hot Start technique, components necessary for amplification are separated so
Works that critical reactants do not mix until reaching a temperature sufficiently high to
suppress primer self-annealing or annealing to nontarget sequences.
Hot Start Options You can perform either a manual Hot Start or an AmpliWax PCR Gem-mediated Hot
Start.
Note
Although manual Hot Start can increase specificity and yield, it is inconvenient and you
can encounter reproducibility and contamination problems.
Performing a Note The manual Hot Start protocol requires the use of mineral oil to prevent evaporation.
Manual Hot Start Thus you cannot perform a manual Hot Start in the GeneAmp PCR systems 2400, 9600, and
9700.
Step
Action
1
Mix all reagents except one key component (choose from dNTPs, MgCl2, or
primers) below a mineral oil cap.
2
Load all tubes into the PCR instrument system.
3
Define temperature control parameters so that the temperature rises to 70–80 °C.
4
Add the missing component to each tube, changing pipet tips after each sample.
continued on next page
Optimizing PCR 6-13
Performing an
AmpliWax PCR
Gem-mediated
Hot Start
Step
Action
1
At room temperature, add primers, MgCl2, dNTPs, and buffer to reaction tube.
2
Add a single AmpliWax PCR Gem to each reaction tube.
Note
The mass of the PCR Gem necessary for proper performance depends
upon the reaction volume and reaction tube geometry.
3
Define temperature control parameters so that the temperature rises to 70–80 °C
for 5–10 minutes, then cools to 2–35 °C.
Note
This creates a wax barrier over the aqueous layer.
4
Add the polymerase and sample buffer above the solid wax layer.
5
Create a PCR thermal profile as follows:
a.
Rapidly heat samples to the first denaturation temperature.
This melts the wax layer, denatures the DNA template, and creates enough
thermal convection to assure complete mixing of all PCR components under
the melted wax. The wax also serves as a vapor barrier during cycling.
6
b.
Program temperature control parameters for conventional thermal cycling.
c.
Cool samples to 2–35 °C at the end of the run.
Run the PCR.
Note
After thermal cycling ends, the wax will form a solid shield preventing
spillage and evaporation.
6-14 Optimizing PCR
7
For post-PCR analysis, you can penetrate the wax layer with a pipet tip and
withdraw the PCR product.
8
Reheat the reaction tube to seal for long-term storage.
Modifying Thermal Cycling Parameters
Guidelines The following table summarizes the effects of modifying temperature control
parameters on PCR performance.
Specific Change in
Thermal Cycling Parameter
Effect on PCR Performance
Raising denaturation temperatures (up to
96 °C)
Can be necessary to allow denaturation,
especially with GC-rich templates
Can also cause template degradation by
depurination
Lowering annealing temperatures
Can increase yield, but can reduce
specificity
Raising annealing temperatures
Increases specificity, but can reduce yield
Setting the denaturation, annealing, and
extension step to at least:
Allows samples to reach thermal equilibrium
at each stage
♦
15 seconds (preferably 30 seconds)
with the GeneAmp PCR System 9600,
9700, or 2400
♦
45 seconds using thin-walled tubes with
the DNA Thermal Cycler 480
♦
1 minute using thick-walled tubes with
the DNA Thermal Cycler 480 or the
DNA Thermal Cycler (TC1)
Using the autoextension (or AutoX) function
of a thermal cycler to allow longer extension
times in later cyclesa
Increases yield by allowing complete
extension of PCR product in later cycles
a. For most applications, an extension temperature of 72 °C is effective and rarely requires optimization. In
the two-temperature PCR process, the combined annealing/extension step temperature should range from
60–70 °C.
Temperature To find the optimal thermal cycling parameters, perform a series of runs varying the
Optimization annealing or denaturation temperatures in 2 °C increments.
Note
Do not vary more than one parameter at a time.
Optimizing PCR 6-15
Avoiding Contamination
Introduction PCR protocols are extremely sensitive to contaminants in the DNA. Although many
protocols that describe “simple” or “fast” extraction or purification methods have been
published recently, you should carefully evaluate any changes or improvements in
extraction or purification methods. (Also, be sure that the physical and chemical
condition of the sample itself are adequate for the intended labeling and assay
methods.)
Avoiding To avoid general contamination, take the following precautionary measures:
Contamination from ♦ Change pipet tips between samples.
the Environment
♦
Use filter-plugged pipet tips.
♦
Clean any work contaminated surface using a cloth soaked with 50% bleach.
IMPORTANT
Before cleaning the sample block of a thermal cycler, refer to the instrument
manual for the proper procedure.
♦
Close sample tubes when not using them.
♦
Always run a no-DNA negative control.
A negative control contains no template DNA, only primers and the DNA diluent (usually
water or buffer).
♦
Aliquot reaction reagents so as to minimize the number of times you use a
particular stock solution.
Avoiding PCR Definition
Product Carryover PCR product carryover is the contamination of an unamplified sample with previously
amplified DNA.
Why Carryover Is a Particular Concern
PCR product carryover is a particular concern because amplified PCR product serves
as an ideal template for subsequent amplifications of that same target.
A single PCR amplification produces a large number of copies (as many as 1013). The
inadvertent transfer of even a minute volume or aerosol of amplified product can mean
significant contamination. This can result in false-positives and the detection and
amplification of the contaminating sequence at the expense of the target sequence.
Precautionary Measures
Adopting these precautionary measures can help you minimize the likelihood of PCR
product carryover.
6-16 Optimizing PCR
♦
Use positive displacement pipettes or filter-plugged pipette tips.
♦
Physically separate reactions prior to and following amplification.
♦
Handle pre- and post-PCR solutions with separate sets of the following:
–
Pipettes
–
Pipette tips
–
Microcentrifuge tubes
–
♦
Gloves
Use AmpErase® UNG in reaction mixtures to prevent the subsequent
reamplification of dU-containing PCR products.
For More Applied Biosystems supplies the GeneAmp PCR Carryover Prevention Kit
Information (P/N N808-0068) and AmpErase UNG (P/N N808-0096) to ensure that PCR products
cannot be reamplified in subsequent PCR amplifications.
Optimizing PCR 6-17
3´ A Nucleotide Addition
Introduction The AmpliTaq and AmpliTaq Gold DNA Polymerases, like many other DNA
polymerases, catalyze the addition of a single nucleotide (usually an adenosine) to the
3´ ends of the two strands of a double-stranded DNA fragment. This non-template
complementary addition results in a denatured PCR product that is one nucleotide
longer than the target sequence. A PCR product containing the extra nucleotide is
referred to as the “plus-A” form.
Why Incomplete 3´ A Nucleotide Addition Can Cause Problems
Because 3´ A nucleotide addition rarely goes to completion without a long extension
step at the end of thermal cycling (i.e., only a fraction of the fragments receive the
extra nucleotide), single-base ladders often form (Figure 6-1), creating peak patterns
that Genotyper® software might not interpret correctly. The resulting allele calls can be
inconsistent, incorrect, or missing entirely, forcing you to inspect all allele calls and to
correct erroneous calls manually.
+A
–A
+A
–A
Figure 6-1 Split peaks resulting from incomplete 3´ A nucleotide addition
How to Avoid Problems Caused by Incomplete 3´ A Nucleotide Addition
♦ Modify the thermal cycling conditions either to promote or to inhibit 3´ A nucleotide
addition.
♦
Modify Mg2+ concentration either to promote or to inhibit 3´ A nucleotide addition.
♦
Modify, or “tail,” the 5´ end of the reverse primer either to promote or to inhibit 3´ A
nucleotide addition to the (forward) labeled strand.
♦
Treat PCR products enzymatically to remove the 3´ A overhangs.
In general, the most reliable strategy is to maximize 3´ A nucleotide addition by
modifying thermal cycling conditions and Mg2+ concentration, and (if necessary) by
tailing the reverse primer.
continued on next page
6-18 Optimizing PCR
Modifying Thermal Increasing the time spent between 60 and 72 °C promotes 3´ A nucleotide addition.
Cycling Conditions Decreasing the time spent between 60 and 72 °C inhibits 3´ A nucleotide addition.
To use this method effectively, you need to determine the optimal thermal cycling
conditions for each marker in each set of reaction conditions.
Promoting 3´ A nucleotide addition has proven to be the more successful strategy.
Residual polymerase activity at room temperature (or even at 4 °C) is often sufficient
to catalyze enough 3´ A nucleotide addition to create genotyping problems. Many
protocols increase the final extension step to 30–45 minutes to promote 3´ A
nucleotide addition.
Modifying Mg2+ Increasing the Mg2+ concentration promotes 3´ A nucleotide addition. Decreasing the
Concentration Mg2+ concentration inhibits plus-A addition.
In general, optimizing the Mg2+ concentration is best employed in conjunction with
other strategies. If you choose to maximize 3´ A nucleotide addition, consider using
AmpliTaq Gold DNA Polymerase at 2.5 mM MgCl2.
Reverse-Primer What It Is
Tailing Brownstein et al. (1996) found that adding additional nucleotides (a “tail”) to the 5´ end
of the reverse PCR primer either promoted or inhibited 3´ A nucleotide addition to the
(forward) labeled strand depending upon the sequence of the added nucleotides.
General Rule
Magnuson et al. (1996) noticed a correlation between tail sequence and the amount of
3´ A nucleotide addition. In particular, they found that adding a single G to the 5´ end
of the reverse PCR primer generally resulted in almost complete 3´ A nucleotide
addition. Therefore, using a tail to promote 3´ A nucleotide addition can yield a
consistently callable pattern.
Things to Consider
Reverse-primer tailing has advantages compared to other methods because it:
♦
Works well under diverse reaction conditions
♦
Does not require additional experimental steps
Enzymatic Ginot et al. (1996) used T4 DNA polymerase to remove the 3´ A overhangs from
Treatment pooled PCR products.
Things to Consider
Although effective, this method has serious limitations because it:
♦
Requires a post-PCR, enzymatic treatment step
♦
Requires titrating each lot of T4 DNA polymerase to determine optimal enzyme
concentrations and treatment times
IMPORTANT
Excess T4 treatment can cause PCR product degradation, whereas
insufficient treatment will fail to correct the problem and can even make some alleles more
difficult to call.
Optimizing PCR 6-19
Specific Suggestion
To begin optimization trials, use 0.5–1 unit of T4 DNA polymerase in 10 µL of pooled
PCR product. Incubate at 37 °C for 30 minutes.
For More Refer to the AmpFl STR Profiler Plus PCR Amplification Kit User’s Manual
Information (P/N 4303501) for more information on maximizing 3´ A nucleotide addition.
Tailed primers are available through the Applied Biosystems Custom Oligonucleotide
Synthesis Service. Call (800)345-5224 for price and availability.
6-20 Optimizing PCR
Stutter Products
What is Stutter? During the PCR amplification of di-, tri-, and tetranucleotide microsatellite loci, minor
products that are 1–4 repeat units shorter than the main allele are produced. The
minor product peaks are referred to as “stutter” peaks. Stutter peaks might be caused
by polymerase slippage during elongation.
Stutter Facts You can estimate the percent stutter by calculating the ratio of the combined heights of
the stutter peaks with the height of the main allele peak. Some general conclusions
about percent stutter follow:
♦
The longer the length of the repeat unit, the less stutter product made
(Figure 6-2).
In other words, among microsatellite loci with the same number of repeat units,
the percent stutter is greater for dinucleotide microsatellite loci than it is for
trinucleotide microsatellite loci, and so on (Walsh et al., 1996).
Figure 6-2 Comparison of the amounts of stutter in dinucleotide (left) and tetranucleotide
(right) repeat loci. Each locus is homozygous, with the largest peak in each picture representing
the “true” allele.
♦
The percent stutter increases with increasing allele length (i.e., with increasing
number of repeat units) as shown in Figure 6-3 on page 6-22.
This rule is likely to be violated if the repeats are not perfect (e.g., if some of the
repeats are partial repeats).
Optimizing PCR 6-21
Figure 6-3 Percent stutter observed for the STR loci in the AmpFl STR Green™ I PCR
Amplification Kit
Evaluating Data The multiband stutter pattern can complicate analysis, particularly of samples with two
with Stutter or more alleles that are close in size. For example, faint bands in a position one repeat
unit smaller than the main allele can be interpreted either as a stutter band or as an
allele in a minor component of a mixed sample. The possibility of stutter makes
precise quantitation especially important to enable the Genotyper software’s filtering
algorithm to interpret the peak pattern accurately.
Fortunately, the percent stutter for a given allele is reproducible. In particular, the
percent stutter does not depend on the quantity of input DNA or the number of loci
amplified during multiplex PCR. The relative invariance of percent stutter is important
for a few reasons:
♦
In many cases, you can adjust the Peak Amplitude Threshold in the Analysis
Parameters window of the GeneScan software so that the analysis program
ignores stutter peaks while recognizing true allele peaks.
♦
Amplifications with an abnormally high percent stutter can indicate mixed samples
(or some other problem with PCR amplification or electrophoresis).
See page 8-25 for examples of stutter patterns in dinucleotide repeat loci.
6-22 Optimizing PCR
Preparing PCR Products for Analysis
Dilution You will almost always need to dilute PCR amplification products before adding them
to the sample tube. Typically, the required dilution lies in the range from 1:3–1:80
(PCR product: distilled, deionized H2O).
A good way to proceed is to begin by optimizing PCR run conditions for your specific
application. Then run a dilution series on your ABI PRISM® 310 Genetic Analyzer to
determine the optimal dilution. Alternatively, run 1 µL of PCR product on a mini-gel. If,
after ethidium bromide staining, the product signal is visible but not oversaturated, try
a 1:10 dilution om your ABI PRISM 310 instrument.
After determining the optimal dilution ratio, you can use the same dilutions for
subsequent analyses as PCR yields should be fairly consistent.
Purification If the expected product length is within 50 nucleotides of the primer length, remove
unincorporated primers before performing electrophoresis. It is often a good idea to
remove unincorporated primers anyway, unless the PCR is run to completion.
Optimizing PCR 6-23
SSCP Analysis
7
7
Overview
About This Chapter This chapter provides detailed instructions for performing Single-Strand Conformation
Polymorphism (SSCP) mutation analysis on the ABI PRISM® 310 Genetic Analyzer.
SSCP analysis is highly sensitive to electrophoresis conditions. The protocol
contained in this section is a good starting point for beginning your own optimization
trials and includes suggestions for improving performance.
This chapter contains the following topics:
Topic
See Page
Introduction to SSCP Analysis
7-2
Before You Begin
7-3
PCR Amplification, Labeling, and Controls
7-4
To Save Time—Prerun Checklist
7-7
Preparing for a Run
7-8
Analyzing the Data
7-12
Optimizing SSCP Run Conditions
7-14
Troubleshooting
7-17
SSCP Analysis 7-1
Introduction to SSCP Analysis
What is SSCP? Single-strand conformation polymorphism (SSCP) analysis is an application that
detects mutations based upon the ability of a single (or multiple) nucleotide change to
alter the electrophoretic mobility of a single-stranded DNA molecule under
non-denaturing conditions.
Under non-denaturing conditions most single-stranded DNA molecules will assume
one or more stable three-dimensional conformations that depend on the nucleotide
sequence. In many cases the change of a single nucleotide will cause a
conformational change that can be detected as a change in the electrophoretic
mobility as compared to the wild type sequence.
Advantages You can analyze a large number of samples using SSCP technique because the
technique is simple and fast. The only step necessary after PCR amplification is a
heat denaturation in formamide and NaOH. Moreover, as with any PCR-based
technique, you can analyze mutations in a specified DNA region by choosing PCR
primers that span that region.
Limitations SSCP analysis indicates only that a mutation exists. You must perform subsequent
DNA sequencing to determine the nature of the mutation that caused an
electrophoretic mobility shift in a given sample.
Moreover, not all point mutations in a given sequence will cause a detectable change
in electrophoretic mobility. However, by optimizing PCR reactions and run conditions
before attempting a large-scale analysis you can increase the sensitivity. (See
“Optimizing SSCP Run Conditions” on page 7-14 for more details.)
Changes in relative mobility due to minor variations in electrophoresis conditions limit
the ability to compare results obtained on different instrument platforms or even in
different laboratories.
Advantages of Using Ability to Vary Electrophoresis Temperature
ABI PRISM The mobility difference between the wild type and a mutant strand is very sensitive to
Technology temperature. Within the temperature range from 25 °C (if your laboratory permits) to
40 °C the temperature for the best differentiation of the two strands will depend upon
the particular mutant/wild type strand combination.
With the ABI PRISM 310 Genetic Analyzer, you can automate electrophoresis of the
same sample at different temperatures. Running the same samples at different
temperatures will maximize your chances of detecting mutations.
Whatever temperature regime you choose, strict temperature control is crucial to
ensure consistency because three-dimensional conformation is highly sensitive to
changes in temperature.
Rapid Analysis
The ABI PRISM 310 Genetic Analyzer allows extremely rapid separations. Fragments
that are 300 bp or less in length can be separated in under 30 minutes. This translates
to a throughput of at least 48 samples in a 24-hour period.
7-2 SSCP Analysis
Before You Begin
Materials Required You will need the following materials to perform an SSCP analysis run.
♦
ABI PRISM Genetic Analyzer Capillary labeled with a green mark (Lt = 47 cm,
Ld = 36 cm, i.d. = 50 µm)
♦
3% GeneScan Polymer (GSP) with 10% (w/w) glycerol and 1X TBE
Note
Optimization might require different polymer concentrations and capillary lengths. See
“5% GeneScan Polymer with 10% Glycerol” on page A-1 for details.
♦
GeneScan Internal Lane Size Standard (recommended: GeneScan-500 or
GeneScan-350)
♦
Deionized formamide
♦
1X TBE buffer containing 10% glycerol
Note
See “1X TBE with 10% Glycerol” on page A-2 for details.
♦
Sodium hydroxide (NaOH), 0.3 N, stored in a plastic container
♦
4.0-mL Genetic Analyzer Vials (do not reuse)
♦
1.0-mL GeneScan Glass Syringe
♦
1.5-mL Eppendorf tube with the lid removed
For a 48-well tray:
♦
0.5-mL Genetic Analyzer Sample Tubes (do not reuse)
♦
Genetic Analyzer Septa for 0.5-mL Sample Tubes (do not reuse)
For a 96-well tray:
♦
0.2-mL MicroAmp® Reaction Tubes (do not reuse)
♦
Genetic Analyzer Septa Strips (do not reuse)
♦
Genetic Analyzer Retainer Clips
Note
The 96-well tray used in the GeneAmp PCR System 9700 requires a tray adaptor to be
used with the ABI PRISM 310 autosampler.
Software You will need the following software to perform and analyze an SSCP run:
Required/Optional ♦ ABI PRISM 310 Collection Software, version 1.0.4 or higher
♦
ABI PRISM Run Module, GS TEMPLATE (A, C, or D)
Use the module that is compatible with the chosen dye set as a template for
creating a dedicated SSCP module.
♦
GeneScan® Analysis Software, version 2.0.2 or higher
We also recommend Genotyper® software, version 2.0. Using Genotyper software,
you can obtain numerical sizing data and use the generated numbers to flag potential
mutations automatically.
SSCP Analysis 7-3
PCR Amplification, Labeling, and Controls
Primer Choice Choose primers so that the resulting PCR product is no longer than 400 (preferably
250) base pairs in length.
Note
Empirical observation indicates that the efficiency of mutation detection is optimal for
fragments between 130 and 250 base pairs in length.
Labeling Rules To use the ABI PRISM™ multicolor fluorescent dye technology for SSCP analysis,
follow these general rules.
Use 5´-End Labeled Primers
The success of SSCP analysis depends upon the ability to detect slight mobility shifts.
The reproducible sizing and sharp peaks obtained when using the 5´-end labeling
method are crucial to the success of this application.
Note
Post-PCR end-labeling with [F]dNTPs is an alternative (Iwahana et al., 1995; Inazuka
et al., 1996; Inazuka et al., 1997).
Use a Different Dye for Each Strand
When you first perform SSCP analysis on a region of DNA you should label the
forward and reverse strands with different dyes. Using different colors for the forward
and reverse strands will permit detection of residual double-stranded molecules
remaining after denaturation, as indicated by overlapping peaks in the two colors. If
you choose not to label both strands, you could mistake a band produced by residual
double-stranded product for a band produced by mutant single-stranded product.
Note
Under certain circumstances both strands can have identical mobilities.
Using a different color for each strand will also allow you to detect mutations that
cause the forward and reverse strands to switch positions without significantly
affecting the relative mobilities of the wild type and mutant samples.
Once data interpretation is well established, differential labeling of the two strands will
not always be necessary. You can switch to using a single dye in order to increase
throughput by running multiple, differently-labeled samples in a single injection.
Dedicate a Color to Each Sample
Because single-stranded DNA molecules can adopt multiple stable conformations,
extra peaks will often be present in an electropherogram. Dedicating a color to each
sample, e.g., labeling the wild type one color and the mutant another, allows you to
confirm the origin of extra peaks.
Label Both Strands
Even if you decide to use a single dye for each sample, it is important that you label
both strands. Labeling both strands increases detection sensitivity and can indicate
potential false-positive results.
Often, mutations will cause an observable mobility shift in only one of the two strands.
By labeling both strands you increase your chances of detecting mutations that affect
the mobility of only one strand.
7-4 SSCP Analysis
Conversely, if a mutation causes only a slight mobility shift in one of the strands, the
likelihood of a false-positive result diminishes if this shift is correlated with a mobility
shift, however slight, in the other strand.
Size Standard A size standard must be defined for each run condition. Many point mutations cause
only slight mobility shifts. Internal lane size standards in a dedicated color greatly
enhance the sensitivity of mutation detection.
We also recommend adding wild type DNA, labeled with the same dye as the size
standard, to the size standard. However, the wild type DNA has to have a similar peak
height to those of the size standard fragments to facilitate peak recognition by the
GeneScan Analysis Software (Inazuka et al., 1997).
Figure 7-1 shows the GeneScan-500 [TAMRA] Internal Lane Size Standard run under
non-denaturing conditions at 25 °C (top panel), 30 °C (middle panel), and 35 °C
(bottom panel).
Figure 7-1 GeneScan-500 [TAMRA] run in 3% GeneScan Polymer with 10% glycerol with 1X
TBE buffer, Lt = 47 cm, 13 kV electrophoresis voltage
Note
The migration rates of the fragments in the size standard do not necessarily conform to
their sizes. The standards are denatured and the resulting single-stranded DNA molecules, like
the samples for analysis, adopt unpredictable three-dimensional conformations. The goal is to
use the size standards to align samples and compare migration rates, not to determine sizes.
continued on next page
SSCP Analysis 7-5
Controls Determining Run-to-run Variation in the Wild Type Sample
Because the mobility shifts caused by many mutations are slight, you must always run
a wild type control to obtain an estimate of injection-to-injection variation in the wild
type sample.
Run 3–5 injections of the wild type sample.
Note
Running five control lanes will allow you to obtain a satisfactory estimate for the
reproducibility under the chosen experimental conditions. Use the values of the five injections to
determine the standard deviation of the wild type sample. Any sample that deviates from the
wild type mean by more than three standard deviations is 99.7% likely to be caused by a
mutation (and not by run-to-run variation in the wild type strand).
Example Control Setup
If you are running 100 injections, run a wild type control every 20th injection. You can
inject from the same sample for all control injections.
Estimate Percent Detectable Mutations
If possible, examine known mutant samples to obtain a rough estimate of percent
detectable mutations before mounting a large-scale analysis. Using the initial set of
electrophoresis conditions described in the following sections, amplify DNA from the
wild type and confirmed mutant samples. Tabulate the percent detectable mutations
for several repeat experiments. If the detection rate is unacceptably low, see the
suggestions for optimizing SSCP run conditions in “Troubleshooting” on page 7-17.
Post-PCR To remove excess primer, purify the amplified PCR product using either a
Purification Step Centricon-100 column (for fragments greater than 130 base pairs in length) or a
Centricon-30 column (for fragments less than 130 base pairs in length).
Note
Performing this step will simplify the analysis. If you do not intend to sequence putative
mutants, this step is not absolutely necessary. However, if you intend to sequence putative
mutants isolated during SSCP analysis, you must perform this purification step.
7-6 SSCP Analysis
To Save Time—Prerun Checklist
Stock Solutions Having stocks of the following reagents/buffers saves time during run setup:
♦
Deionized formamide
Lasts for three months at –15 to –25 °C. See “Deionized Formamide” on page A-3
for details.
♦
Sodium hydroxide (NaOH), 0.3 N, stored in a plastic container at room
temperature
♦
Formamide/NaOH/Size Standard Master Mix
Lasts for one week at 2–6 °C. See step 2 on page 7-8 for details.
♦
3% GeneScan Polymer (GSP) with 10% glycerol in 1X TBE
Lasts for 3 months at room temperature. See “5% GeneScan Polymer with 10%
Glycerol” on page A-1 for details.
♦
1X TBE buffer with 10% glycerol
Lasts for 3 month at room temperature. On the instrument, the buffer lasts for 48
hours or 100 injections, whichever comes first. See “1X TBE with 10% Glycerol”
on page A-2 for details.
At the Beginning Set the instrument run temperature to the desired temperature (30 °C by default)
of a Run immediately before run setup. Refer to the ABI PRISM 310 Genetic Analyzer User’s
Manual for details.
At Any Time Before Perform the following at any time before running:
a Run ♦ Complete the Sample Sheet.
Refer to the GeneScan Analysis Software User’s Manual for details.
♦
Create an SSCP analysis matrix file.
For directions on preparing matrix samples for SSCP analysis, see page 7-9. See
Appendix B for instructions on creating a matrix file. Usually, you create and then
reuse a single matrix file for each set of run conditions.
SSCP Analysis 7-7
Preparing for a Run
Instrument Setup Refer to the ABI PRISM 310 Genetic Analyzer User’s Manual for the general
procedure.
The specific equipment, polymers, and buffers needed for an SSCP analysis run are
listed in “Before You Begin” on page 7-3.
Preparing and Preparing and Loading Experimental Samples
Loading Samples Note Sometimes you will need to dilute the PCR product in distilled, deionized H O before
2
loading 1 µL into the sample tube.
To prepare and load the samples:
Step
Action
1
Label the 0.5-mL (48-well tray) or 0.2-mL (96-well tray) sample tubes with a
permanent marker.
2
To each tube add:
♦
10.5 µL deionized formamide
♦
1 µL GeneScan Internal Lane Size Standard (GeneScan-350 or
GeneScan-500 recommended)
♦
1 µL PCR product
♦
0.5 µL 0.3 N NaOH (added to the samples to keep them denatured for
extended periods of time)
! WARNING ! CHEMICAL HAZARD. Formamide is a known teratogen. It
can cause birth defects. Wash thoroughly after handling formamide. Obtain a
copy of the MSDS from the manufacturer. Wear appropriate protective
eyewear, clothing, and gloves. Wash thoroughly after handling formamide.
! WARNING ! CHEMICAL HAZARD. Sodium hydroxide (NaOH) can cause
severe burns to the skin, eyes, and respiratory tract. Always work in a fume
hood. Obtain a copy of the MSDS from the manufacturer. Wear appropriate
protective eyewear, clothing, and gloves.
Note
For convenience, you can combine the formamide, NaOH, and GeneScan
Size Standard into a master mix (1050 µL deionized formamide + 50 µL 0.3 N
NaOH + 100 µL GeneScan Size Standard). This mix will last for 1 week at 2–6 °C.
Aliquot 12 µL of the mix into each sample tube before adding 1 µL of PCR product.
3
Seal each tube with a septum, taking care to insert the septum completely.
4
Are you using a 48- or a 96-well sample tray?
♦
If you are using a 48-well sample tray, skip to step 5.
♦
If you are using a 96-well sample tray, insert the tubes into the tray and then go
to step 5.
You can denature and cool the samples directly in the tray. For directions refer
to the Genetic Analyzer Septa Strip and Retainer Clip User Bulletin
(P/N 904512).
7-8 SSCP Analysis
5
Place the samples in a heat block or thermal cycler for 5 minutes at 95 °C.
6
Remove the tubes from the heat source and place immediately in an ice-water bath.
To prepare and load the samples:
Step
7
8
(continued)
Action
Are you using a 48- or a 96-well sample tray?
♦
If you are using a 48-well sample tray, insert the tubes into the tray and then go
to step 8.
♦
If you are using a 96-well sample tray, skip to step 8.
Place the sample tray on the autosampler.
Note
The 96-well tray used in the GeneAmp PCR System 9700 requires a tray
adaptor to be used with the ABI PRISM 310 autosampler.
Preparing the Matrix Samples
Step
1
Action
Prepare the matrix samples by adding 10.5 µL of deionized formamide, 0.5 µL of
0.3 N NaOH, and 1 µL of one of the matrix standards (Dye Primer or Fluorescent
Amidite, see page 7-12) to each of four sample tubes.
! WARNING ! CHEMICAL HAZARD. Formamide is a known teratogen. It
can cause birth defects. Wash thoroughly after handling formamide. Obtain a
copy of the MSDS from the manufacturer. Wear appropriate protective
eyewear, clothing, and gloves. Wash thoroughly after handling formamide.
! WARNING ! CHEMICAL HAZARD. Sodium hydroxide (NaOH) can cause
severe burns to the skin, eyes, and respiratory tract. Always work in a fume
hood. Obtain a copy of the MSDS from the manufacturer. Wear appropriate
protective eyewear, clothing, and gloves.
2
Place the samples in a heat block or thermal cycler for 5 minutes at 95 °C.
3
Remove the tubes from the heat source and place immediately in an ice-water bath.
4
Run these four injections either alone or in the first four injections of an
experimental run.
Creating the Currently no dedicated SSCP module exists for the ABI PRISM 310 Genetic Analyzer.
Run Module You will need to duplicate and edit one of the template modules.
To create the run module:
Step
Action
1
Open the Modules folder (located in the ABI PRISM 310 folder).
2
Duplicate one of the GS TEMPLATE modules and rename the new module
GS SSCP A (or C or D), as appropriate.
Note
The proper template module depends upon the dye set you are using. Use
module GS TEMPLATE A with dye primers and module GS TEMPLATE C or
GS TEMPLATE D with fluorescent amidites (see Table 4-3 on page 4-6 and
“Creating a Matrix File” on page 7-12).
3
Double-click the ABI PRISM 310 Collection icon if the program is not currently open.
4
Select your module from step 2 in the Manual Control window.
SSCP Analysis 7-9
To create the run module:
Step
5
(continued)
Action
Specify the settings as shown below.
5–10
5–15
15–25
9–15
Note
Choose injection times between 5 and 10 seconds and collection times
between 15 and 25 minutes depending upon the polymer concentration,
electrophoresis voltage, and size of your samples.
Note
The Syringe Pump Time setting is for a 47-cm capillary filled with 3%
GeneScan Polymer. Other capillary length and polymer concentration combinations
might require different pump times (see Table 7-1 on page 7-17).
6
Click on Save As Default to save the GS SSCP module settings.
;
Starting the Run
To start the run:
Step
Action
1
If you have installed a new capillary and have not already reset the injection counter
to zero, select Change Capillary from the Instrument window. Then click OK in the
Reset window.
2
Set up the Sample Sheet as described in the ABI PRISM 310 Genetic Analyzer
User’s Manual.
Note
You can prepare the Sample Sheet at any time prior to the run and save it
to the Sample Sheet folder.
3
Select New from the File pull-down menu and click the GeneScan™ Injection List
icon.
4
Set up the Injection List as described in the ABI PRISM 310 Genetic Analyzer User’s
Manual.
Be sure to do the following:
♦
Select the appropriate Sample Sheet from the Sample Sheet pop-up window.
♦
Select module GS SSCP from the Module pop-up menu for every injection.
♦
If available, select the appropriate matrix file from the Matrix pop-up window for
every injection.
Note
If you have not already created a matrix file, see “Preparing the Matrix
Samples” on page 7-9 and Appendix B. You can still start the run and assign the
matrix to the sample files later.
7-10 SSCP Analysis
To start the run:
Step
5
(continued)
Action
Click the Start button.
Note
If you have not preheated the heat plate, the module has an initial step in
which the plate is heated to the selected run temperature before the first sample is
run.
SSCP Analysis 7-11
Analyzing the Data
Creating a You must create a matrix file before analyzing SSCP data for the first time. For more
Matrix File information on creating matrices, see Appendix B.
For directions on preparing matrix samples for SSCP analysis, see page 7-9. Make
sure that you denature the matrix samples before loading.
To create the matrix file, use one of the following:
♦
Dye Primer Matrix Standards Kit (5-FAM, JOE, TAMRA, and ROX, P/N 401114)
and module GS SSCP A
♦
Fluorescent Amidite Matrix Standards Kit (6-FAM, TET, HEX, and TAMRA,
P/N 401546) and module GS SSCP C
♦
Fluorescent Amidite Matrix Standards Kit (6-FAM, HEX, and ROX, P/N 401546),
the NED Matrix Standard (P/N 402996), and module GS SSCP D
Name the new matrix SSCP Matrix A, SSCP Matrix C, or SSCP Matrix D as
appropriate.
Note
Usually, you create and save a single matrix file for each set of run conditions.
However, if you experience persistent problems, such as spectral overlap in the analyzed data,
you should remake the matrix file even if you have not altered the run conditions.
Setting the Analysis IMPORTANT
If you choose to use different analysis parameters from those recommended
Parameters here, be sure to define the Analysis Range to exclude the primer peak.
To set the analysis parameters:
Step
Action
1
Open the GeneScan Analysis Software (version 2.0.2 or higher).
2
Choose New from the File menu and click the Analysis Parameters icon.
3
Specify the settings as shown below.
IMPORTANT
The Analysis Range will vary with polymer concentration and
temperature. The setting shown is for 3% GeneScan Polymer at 30 °C.
4
7-12 SSCP Analysis
Choose Save As... from the File menu.
To set the analysis parameters:
Step
(continued)
Action
5
Save the settings as “SSCP Analysis Parameters.”
6
Click OK when done.
Analyzing For brief directions on analyzing sample files, see page 3-2.
Sample Files
Refer to the GeneScan Analysis Software User’s Manual for detailed protocols.
SSCP Analysis 7-13
Optimizing SSCP Run Conditions
Sensitivity to Run SSCP analysis is more sensitive to electrophoresis conditions than many ABI PRISM
Conditions applications. You should optimize run conditions for your particular system.
Of the factors affecting electrophoretic mobility under non-denaturing conditions, only
capillary length and polymer concentration have a predictable effect. Increasing either
capillary length or polymer concentration will increase the separation between the wild
type and mutant strands.
The following factors have an unpredictable or undetermined effect on electrophoretic
mobility under non-denaturing conditions. Therefore many of the optimization
suggestions contained here are empirically derived.
♦
Glycerol (or other cosolvent) percentage in polymer
♦
Fragment size
♦
Mutation position within the DNA region of interest
♦
Buffer pH
♦
Electrophoresis voltage
♦
Run temperature
Capillary Length Because many of the mobility shifts in mutants are slight, increasing the length of the
capillary increases the detection power. Increasing the capillary length also increases
both the capillary fill time and the run time.
Polymer Within the range of 1–5% GeneScan Polymer concentration, experimental results
Concentration indicate that increasing polymer concentration increases detection power (Inazuka
et al., 1997).
♦
Begin your trials using 3% GeneScan Polymer:
♦
If your results are poor, increase the polymer percentage to as much as 5%.
♦
If your results are good, to save time decrease the polymer concentration to as
little as 1% as long as the percentage of detectable mutations continues to be
acceptable.
Increasing the polymer concentration also increases both the capillary fill time and the
run time.
continued on next page
7-14 SSCP Analysis
Glycerol Percentage Glycerol at concentrations of 5–10% usually stabilizes three-dimensional DNA
conformations and thus enhances mutation detection.
Begin your trials using 10% glycerol. If you decide to alter glycerol concentration, try
concentrations in the range from 5–10%.
Other possible cosolvents you might want to consider include the following (Glavac
and Dean, 1993):
♦
Urea
♦
Formamide
♦
Sucrose
♦
Glucose
♦
DMSO
Fragment Size If your results are poor and the fragment length is well outside the optimal size range
of 130–250 bp, consider choosing new primers so that the fragment length is within
the optimal size range.
Hayashi et al. (1992) found that at least 90% of single base-pair substitutions can be
detected if the PCR products are kept under 200 bp in length and that 80% of single
base-pair substitutions can be detected if the PCR products are kept under 400 bp in
length.
Inazuka et al. (1997) found that the ABI PRISM 310 Genetic Analyzer can be used to
analyze fragments up to 741 bp.
Mutation Position A given point mutation will interact differently with the various regions in the
surrounding DNA. Changing the primer positions to amplify different regions of the
surrounding DNA can change the relative mobility difference between the mutant and
the wild type fragments.
Buffer pH Kukita et al. (1997) suggest that low pH greatly increases the sensitivity of mutation
detection in a slab gel format, enabling effective analysis of fragments as large as
800 bp in length.
Electrophoresis Within the range from 9–15 kV, a slight drop-off in detectability is apparent at or above
Voltage 13 kV (perhaps due to a destabilizing effect of high electric-field strengths on
three-dimensional conformation).
Begin your trials with an electrophoresis voltage of 15 kV. If your results are poor,
consider decreasing the voltage to as little a 9 kV.
Note
Decreasing electrophoresis voltage increases run time.
continued on next page
SSCP Analysis 7-15
Run Temperature The ABI PRISM 310 Genetic Analyzer has no mechanism for capillary cooling. In
general, cooler temperatures stabilize three-dimensional conformation and thus
enhance detectability. If your lab permits, try run temperatures below 30 °C.
Sometimes, however, raising the temperature above 30 °C improves results. 40–45 °C
appears to be an empirical upper limit to improving performance (Atha et al., 1998).
Figure 7-2 shows mobility differences between p53 mutant and wild type SSCP
samples at 25 °C, 30 °C, and 35 °C for both forward (blue) and reverse strands
(green). The Namalwa sample (left) gives the best differentiation between wild type
and mutant at 25 °C, the H596 sample (middle) gives the best differentiation at 30 °C,
and the Colo320 sample (right) gives the best differentiation at 35 °C.
Figure 7-2 Temperature dependence of p53 mutant and wild type SSCP mobility profiles. Mutant sample mobilities are
given as differences in number of data points from the wild type sample mobilities (defined as zero). Forward strands are
shown in blue and reverse strands are shown in green.
7-16 SSCP Analysis
Troubleshooting
Preventing Problems As with any high-resolution application, it is advisable to display the migration time of
at least one size standard peak for every injection. Verify that the migration times of
the size standard peaks are similar from injection to injection before flagging a
potential mutant. This will decrease the number of false-positive results.
Size Standards Because of the complex peak patterns of the internal lane size standards that are
often seen in SSCP runs, it can be difficult for the GeneScan Analysis Software’s
peak-detection algorithm to recognize peaks reproducibly.
♦
Examine your data for each injection to ensure that the correct peaks are being
called.
♦
Adjust the Peak Height Threshold in the Analysis Parameters window to get the
most consistent data.
♦
Define the size standard so that each unknown peak is flanked by at least two size
standard peaks on either side.
♦
Adjust the values in the Analysis Range section of the Analysis Parameters
window to include only the peaks of interest.
Sodium Hydroxide Using poor-quality or old sodium hydroxide solutions can lead to decreased capillary
lifetimes.
IMPORTANT
Do not store sodium hydroxide in glass bottles. NaOH etches glass.
Syringe Pump Times When you change any of the following parameters, you must also change the Syringe
Pump Time (in the GS SSCP module settings) accordingly:
♦
Capillary length
♦
Polymer concentration
♦
Glycerol (or other co-solvent) percentage
Table 7-1 illustrates the effect of capillary length, polymer concentration, and glycerol
presence on fill time at 30 °C.
Table 7-1 Syringe Pump Times
Fill Time (sec.) for various GeneScan Polymer Concentrations
Lt (cm)
10%
Glycerol
1%
3%
5%
47
no
10
20
50
47
yes
25
30
60
61
yes
30
40
100
♦
When using low polymer concentrations, if the Syringe Pump Time is too long, you
may run out of polymer.
♦
When using high polymer concentrations, if the Syringe Pump Time is too short,
the capillary is not completely filled. Runs get progressively slower (i.e., size
standard peaks come off at higher and higher scan numbers).
continued on next page
SSCP Analysis 7-17
Laboratory The laboratory temperature should be maintained between 15 and 30 °C. Once the
Temperature and ABI PRISM 310 Genetic Analyzer is set up and in operation, the laboratory
Humidity temperature should not fluctuate more than ±2 °C.
The instrument can tolerate up to 80% non-condensing relative humidity. Avoid
placing it near heaters, cooling ducts, or heat-producing instruments.
7-18 SSCP Analysis
Microsatellite Analysis 8
8
Overview
In This Chapter This chapter provides detailed instructions for performing microsatellite analysis with
the Performance Optimized Polymer 4 (POP-4™) on the ABI PRISM® 310 Genetic
Analyzer.
This chapter contains the following topics:
Topic
See Page
Introduction to Microsatellite Analysis
8-2
Before You Begin
8-3
PCR Amplification, Labeling, and Controls for Microsatellite Analysis
8-4
To Save Time—Prerun Checklist
8-6
Preparing for a Run
8-7
Analyzing the Data, Part I—Using GeneScan
8-10
Analyzing the Data, Part II—Allele Binning Using Genotyper 2.0
8-12
Troubleshooting Microsatellite Analysis
8-25
Microsatellite Analysis 8-1
Introduction to Microsatellite Analysis
Definition Microsatellite markers, also called short tandem repeat (STR) markers, are
polymorphic DNA loci that contain a repeated nucleotide sequence. The repeat unit
can be from 2–7 nucleotides in length. The number of nucleotides per repeat unit is
the same for a majority of repeats within a microsatellite locus.
What is Microsatellite loci are PCR amplified and the PCR products are then analyzed by
Microsatellite electrophoresis to separate the alleles according to size. PCR-amplified microsatellite
Analysis? alleles can be detected using various methods, such as fluorescent dye labeling, silver
staining, or fluorescent dye staining.
Background The number of repeat units at a microsatellite locus may differ, so alleles of many
different lengths are possible. Microsatellite loci occur throughout the genome of most
organisms and therefore have been used as markers to establish linkage groups in
crosses and to map genetically identified mutations to chromosomal positions.
If allele frequencies are known, highly polymorphic microsatellite loci are very useful
for identifying individuals in a population and for determining the probability that two
individuals are related. Their even distribution in the genome makes them very good
markers for constructing genetic maps (Edwards et al., 1992).
Advantages of PCR-based microsatellite analysis has the following advantages over conventional
PCR-Based genotyping methods, e.g., Restriction Fragment Length Polymorphism (RFLP):
Microsatellite ♦ The small size of microsatellite loci improves the chance of obtaining a result,
Analysis
particularly for samples containing minute amounts of DNA and/or degraded DNA.
♦
The small size range of microsatellite loci makes them ideal candidates for
co-amplification while keeping all amplified alleles smaller than 350 base pairs.
Many microsatellite loci can therefore be typed from a single PCR.
♦
Microsatellite alleles have discrete sizes, allowing for simplified interpretation of
results.
♦
PCR-based tests are rapid, giving results in 24 hours or less.
♦
PCR-based tests are easy to standardize and automate, ensuring reproducible
results.
Advantages of Using To exploit the potential for increased throughput using ABI PRISM™ multicolor
ABI PRISM fluorescent dye technology, you can multiplex electrophoresis by co-loading the
Technology products of multiple PCR reactions during the same capillary injection.
The ABI PRISM 310 Genetic Analyzer allows extremely rapid separations: fragments
that are 450 base pairs or less in length can be separated in under 30 minutes. This
translates to a throughput of up to 48 samples in a 24-hour period.
8-2 Microsatellite Analysis
Before You Begin
Materials Required You will need the following materials to perform a microsatellite analysis run.
♦
Performance Optimized Polymer 4 (POP-4)
♦
ABI PRISM Genetic Analyzer Capillary labeled with a green mark (Lt = 47 cm,
Ld = 36 cm, i.d. = 50 µm)
♦
GeneScan Internal Lane Size Standard (recommended: GeneScan-350,
GeneScan-400 HD, or GeneScan-500)
♦
Genetic Analyzer Buffer with EDTA
♦
4.0-mL Genetic Analyzer Vials (do not reuse)
♦
1.0-mL or 2.5-mL GeneScan Glass Syringe
♦
1.5-mL Eppendorf tube with the lid removed
For a 48-well tray:
♦
0.5-mL Genetic Analyzer Sample Tubes (do not reuse)
♦
Genetic Analyzer Septa for 0.5-mL Sample Tubes (do not reuse)
For a 96-well tray:
♦
0.2-mL MicroAmp® Reaction Tubes (do not reuse)
♦
Genetic Analyzer Septa Strips (do not reuse)
♦
Genetic Analyzer Retainer Clips
Note
The 96-well tray used in the GeneAmp PCR System 9700 requires a tray adaptor to be
used with the ABI PRISM 310 autosampler.
Software Required You will need the following software to perform and analyze a microsatellite analysis
run:
♦
ABI PRISM 310 Collection Software, version 1.0.4 or higher
♦
ABI PRISM Run Module, GS STR POP4 (A,C, D, or F) (1.0 or 2.5 mL).
Be sure to use the version that is compatible with the chosen dye set.
♦
GeneScan® Analysis Software, version 2.0.2 or higher
♦
Genotyper® Software, version 2.0
Microsatellite Analysis 8-3
PCR Amplification, Labeling, and Controls for Microsatellite Analysis
PCR Amplification Reactant Concentrations and Volumes
The following table provides guidelines for beginning multiplex PCR in your system. In
many systems, the 7.5-µL reaction volume produces sufficient product without
extensive optimization.
Table 8-1 Preparing PCR Reaction Mixtures
Volume (µL)
(15-µL rxn)
Volume (µL)
(7.5-µL rxn)
1.20
(50 ng/µL stock)
1.20
(25 ng/µL stock)
PCR Primer Mix (5 µM each primer)
1.00
0.50
10X GeneAmp® PCR Buffer II
1.50
0.75
GeneAmp dNTP Mix (250 µM each dNTP)
1.50
0.75
AmpliTaq Gold™ DNA Polymerase
(5 U/µL)
0.12
0.06
MgCl2 (25 mM)
1.50
0.75
Distilled, deionized H2O
8.18
3.49
Reaction Component
DNAa
a. Applied Biosystems recommends adding the same volume of template DNA to the 15-µL and 7.5-µL
reactions because manual pipetting of volumes smaller than 1 µL is inaccurate.
IMPORTANT
To avoid the inaccuracies associated with pipetting small volumes, you should
combine all reaction components except sample DNA in a PCR Master Mix. Using the ratios in
the preceding table, prepare sufficient mix for at least one extra reaction volume. Aliquot 13.8 µL
of the mix into each 15-µL reaction or 6.3 µL of the mix into each 7.5-µL reaction. PCR Master
Mix lasts for 1–2 weeks at 2–6 °C.
Thermal Cycling Profile
The following table lists recommended thermal cycling times and temperatures on a
GeneAmp® PCR System 2400, 9600, or 9700 for both the 15- and 7.5-µL reactions.
Initial
Incubation
Step
Each of 10 Cycles
Melt
HOLD
Anneal
Extend
Each of 20 Cycles
Melt
CYCLE
95 °C
12 min.
94 °C
15 sec.
55 °C
15 sec.
Anneal
Extend
CYCLE
72 °C
15 sec.
89 °C
15 sec.
55 °C
15 sec.
72 °C
15 sec.
Final
Extension
Final
Step
HOLD
HOLD
72 °C
10 min.
4 °C
(forever)
If some loci amplify poorly, see “Multiplexing PCR” on page 6-10 and “Troubleshooting
PCR Amplification” on page 11-1 for suggestions on improving PCR performance.
continued on next page
8-4 Microsatellite Analysis
Labeling Rules Use 5´-end labeled primers. The success of microsatellite analysis depends upon the
ability to detect small mobility differences. The reproducible sizing and sharp peaks
obtained when using the 5´-end labeling method are crucial to the success of this
application.
Size Standard Always use a GeneScan Internal Lane Size Standard.
Control DNA In this context, control DNA satisfies the following criteria:
♦
The DNA comes from a single individual with known genotype.
♦
The DNA sample is in sufficiently good condition to serve as a positive control for
PCR amplification.
Applied Biosystems recommends using control DNA (such as the CEPH 1347-02
standard used to generate the Généthon map of the human genome) to monitor
several stages of the experimental process. Control DNA:
♦
Serves as a positive control for troubleshooting PCR amplification
For example, if the sample DNA amplifies poorly, knowing whether the control
DNA amplifies will allow you to distinguish between problems with the sample
DNA (control DNA amplifies) and problems with reagents, instruments, or
protocols (control DNA does not amplify).
♦
Serves as a sizing reference for monitoring injection-to-injection and
capillary-to-capillary variation
Because the control DNA is not used to calculate the sizing curve, the size
obtained for the control DNA across gels will alert you to potential problems with
sizing precision.
♦
Facilitates allele binning
Allele binning is a simple statistical method for converting peak sizes to alleles.
Briefly, the method involves generating a frequency histogram of called sizes.
Refer to the Genotyper User’s Manual for a detailed discussion of allele binning.
IMPORTANT
To convert a fragment’s called size to an allele, you cannot simply round the
called size to the nearest allele size.
If you choose a commonly-used standard such as CEPH 1347-02 (P/N 403062), you
can correlate the allele sizes that you obtain with the allele sizes obtained by others,
such as the CEPH Genotype Database (http://www.cephdb.fr/cephdb).
For more information on the CEPH Genotype Database, refer to page 7-33 of the
ABI PRISM Linkage Mapping Set Version 2 User’s Manual.
You can also use an allelic ladder to genotype analyzed samples (see page 9-23).
Guidelines for Using Control DNA
Amplify at least one control DNA sample for every round of PCR amplification.
Run at least one injection of amplified control DNA for every set of microsatellite
markers used. Run at least one injection of amplified control DNA whenever you
change the capillary or electrophoresis conditions.
Microsatellite Analysis 8-5
To Save Time—Prerun Checklist
\
Stock Solutions Having stocks of the following reagents/buffers saves time during run setup:
♦
Deionized formamide
Lasts for 3 months at –15 to –25 °C. See “Deionized Formamide” on page A-3 for
details.
♦
Formamide/Size Standard Master Mix
Lasts for 2 weeks at 2–6 °C. See step 2 on page 8-7 for details.
♦
1X Genetic Analyzer Buffer with EDTA
Lasts for 2 weeks at 2–6 °C and for 48 hours or 100 injections, whichever comes
first, on the instrument.
At the Beginning of a Perform the following immediately before run setup:
Run ♦ Allow the POP-4 polymer to warm to room temperature.
♦
Set the instrument run temperature to 60 °C.
Refer to the ABI PRISM 310 Genetic Analyzer User’s Manual for details.
At Any Time Before Perform the following at any time before running:
a Run ♦ Complete the Sample Sheet.
Refer to the GeneScan Analysis Software User’s Manual for details.
♦
Create a microsatellite analysis matrix file.
For directions on preparing matrix samples for microsatellite analysis, see
page 8-8. See Appendix B for instructions on creating a matrix file. Usually, you
create and then reuse a single matrix file for each set of run conditions.
8-6 Microsatellite Analysis
Preparing for a Run
Instrument Setup Refer to the ABI PRISM 310 Genetic Analyzer User’s Manual for the general
procedure.
The specific equipment, polymers, and buffers needed for microsatellite analysis run
are listed in “Before You Begin” on page 8-3.
Preparing and Note Sometimes you will need to dilute the PCR product 1:10 in distilled, deionized H2O
Loading Samples before loading 1 µL into the sample tube.
Step
Action
1
Label the 0.5-mL (48-well tray) or 0.2-mL (96-well tray) sample tubes with a
permanent marker.
2
To each tube add the following:
♦
12 µL deionized formamide
♦
0.5 µL GeneScan Internal Lane Size Standard
♦
1 µL PCR product
! WARNING ! CHEMICAL HAZARD. Formamide is a known teratogen. It
can cause birth defects. Wash thoroughly after handling formamide. Obtain a
copy of the MSDS from the manufacturer. Wear appropriate protective
eyewear, clothing, and gloves. Wash thoroughly after handling formamide.
Note
For convenience, you can combine the formamide and GeneScan Size
Standard into a master mix (1200 µL deionized formamide + 50 µL GeneScan Size
Standard). Put 12.5 µL of the mix and 1 µL of PCR product into each sample tube.
This mix will last for 2 weeks at 2–6 °C.
3
Seal each tube with a septum, taking care to insert the septum completely.
4
Are you using a 48- or a 96-well sample tray?
♦
If you are using a 48-well sample tray, skip to step 5.
♦
If you are using a 96-well sample tray, insert the tubes into the tray and then go
to step 5.
You can denature and cool the samples directly in the tray. For directions refer
to the Genetic Analyzer Septa Strip and Retainer Clip User Bulletin
(P/N 904512).
5
Place the samples in a heat block or thermal cycler for 5 minutes at 95 °C.
6
Remove the tubes from the heat source and place immediately in an ice-water bath.
7
Are you using a 48- or a 96-well sample tray?
8
♦
If you are using a 48-well sample tray, insert the tubes into the tray and then go
to step 8.
♦
If you are using a 96-well sample tray, skip to step 8.
Place the sample tray on the autosampler.
Note
The 96-well tray used in the GeneAmp PCR System 9700 requires a tray
adaptor to be used with the ABI PRISM 310 autosampler.
Microsatellite Analysis 8-7
Preparing the Matrix Samples
Step
1
Action
Prepare the matrix samples by adding 12 µL of deionized formamide and 1 µL of
one of the matrix standards (Dye Primer or Fluorescent Amidite) to each of four
sample tubes.
! WARNING ! CHEMICAL HAZARD. Formamide is a known teratogen. It
can cause birth defects. Wash thoroughly after handling formamide. Obtain a
copy of the MSDS from the manufacturer. Wear appropriate protective
eyewear, clothing, and gloves. Wash thoroughly after handling formamide.
2
Denature the samples for 5 minutes at 95 °C.
3
Cool the samples by placing directly on ice.
4
Run these four injections, either alone or in the first four injections of an
experimental run.
Starting the Run Note
Run module GS STR POP4 permits detection of the 400-bp peak of the
GeneScan-500 size standard. By increasing the run time from 24 minutes to 26 minutes, you
can also detect the 500-bp peak of the GeneScan-500 size standard.
To start the run:
Step
Action
1
Double-click the ABI PRISM 310 Collection icon if the program is not currently open.
2
If you have installed a new capillary and have not already reset the injection counter
to zero, select Change Capillary from the Instrument window. Then click OK in the
Reset window.
3
Set up the Sample Sheet as described in the ABI PRISM 310 Genetic Analyzer
User’s Manual.
Note
You can prepare the Sample Sheet at any time before the run and save it
to the Sample Sheet folder.
4
From the File pull-down menu, select New and click the GeneScan Injection List
icon.
5
To increase the run time from 24 minutes to 26 minutes:
a.
Select run module GS STR POP4 from the Manual Control window.
b.
Type 26 in the Collection Time data field.
c.
Click Use Settings.
Note
only.
6
The Use Settings button will store the settings for the current Injection List
Set up the Injection List as described in Chapter 4 of the ABI PRISM 310 Genetic
Analyzer User’s Manual.
Be sure to do the following:
a.
Select the appropriate Sample Sheet from the Sample Sheet window.
b.
Select run module GS STR POP4 from the Module pop-up menu for every
injection.
c.
If available, select the appropriate matrix file from the Matrix window for every
injection.
Note
If you have not already created a matrix file, see page 8-8 and
Appendix B. You can still start the run and assign the matrix to the sample files later.
8-8 Microsatellite Analysis
To start the run:
Step
7
(continued)
Action
Click Start.
Note
If you have not preheated the heat plate, the module has an initial step in
which the plate is heated to 60 °C before the first sample is run.
Microsatellite Analysis 8-9
Analyzing the Data, Part I—Using GeneScan
After A Run: The following diagram summarizes the data analysis process using the GeneScan
Process Overview Analysis software. Setting the analysis parameters is covered in more detail on
page 8-11. For brief directions on analyzing sample files, see page 3-2.
Open the project file
Install a new matrix if necessary
Set the Analysis Parameters
Define the size standard
Analyze the data
Creating a New You must create a matrix file before analyzing microsatellite data for the first time. For
Matrix File more information on creating matrix files, see Appendix B.
For directions on preparing matrix samples for microsatellite analysis, see “Preparing
the Matrix Samples” on page 8-8. To create the matrix file, use one of the following:
♦
Dye Primer Matrix Standards Kit (5-FAM, JOE, TAMRA, and ROX, P/N 401114)
and module GS STR POP4 A
♦
Fluorescent Amidite Matrix Standards Kit (6-FAM, TET, HEX, and TAMRA,
P/N 401546) and module GS STR POP4 C
♦
Fluorescent Amidite Matrix Standards Kit (6-FAM, HEX, and ROX, P/N 401546),
the NED Matrix Standard (P/N 402996), and module GS STR POP4 D
♦
Dye Primer Matrix Standards Kit (5-FAM, JOE, and ROX, P/N 401114), the NED
Matrix Standard (P/N 402996), and module GS STR POP4 F
Note
Usually, you create and save a single matrix file for each set of run conditions.
However, if you experience persistent problems, such as spectral overlap in the analyzed data,
you should remake the matrix file even if you have not altered the run conditions.
continued on next page
8-10 Microsatellite Analysis
Setting the Analysis
Parameters
Step
1
Action
Open the GeneScan Analysis Software (version 2.0.2 or higher).
2
From the File menu, choose New and click the Analysis Parameters icon.
3
Specify the settings as shown below.
Note
The primer peak is usually detected in the 2600–3000 scan number range.
You should start the analysis range immediately after the primer peak in order to
see only the size standard and microsatellite data. Examine the raw data to
determine the exact position of the primer peak.
4
Choose Save As... from the File menu.
5
Save the settings as Microsatellite Analysis Parameters.
6
Click OK when done.
Analyzing For brief directions on analyzing sample files, see page 3-2.
Sample Files
The GeneScan Analysis Software User’s Manual contains detailed protocols.
Microsatellite Analysis 8-11
Analyzing the Data, Part II—Allele Binning Using Genotyper 2.0
What is Allele Allele definitions for microsatellite markers are based on the fragment length (size) of
Binning? the PCR products as estimated by gel or capillary electrophoresis. Experimental
variation in sizing has led to the practice of “binning” alleles—grouping allele
fragments belonging to a particular size into a range (bin) centered around the
average size with a tolerance limit. A typical allele definition would look like this:
101.5 ± 0.5 bp.
Benefits of Allele Allele binning has several benefits:
Binning ♦ As the sample size increases for a particular marker or set of markers, new or
previously undefined alleles can appear in the sample. Allele binning helps you to
accommodate undefined alleles.
♦
Allele sizes tend to vary among electrophoresis runs due to subtle differences in
gels or capillaries and electrophoresis conditions. Allele binning allows you to
define appropriate tolerances for this variance.
♦
You can define alleles more precisely by binning alleles based on sample size.
♦
If using the same control DNA (e.g., CEPH 1347-02) on every run, you can adjust
allele definitions against the reference alleles automatically by binning alleles.
Methods Used to Bin You can perform allele binning using any of the following Genotyper 2.0 features:
Alleles ♦ Histogram window
♦
Plot window
♦
Make from Labels…
♦
Add Multiple Categories…
♦
Offset/Calculate Offset…
In general, we recommend using the Histogram window for binning alleles. This
method works best when the full data set from a study is available for each marker
before the allele bins are determined.
Note
For users of the ABI PRISM Fluorescent Genotyping Demonstration Kit—To familiarize
yourself with the allele binning methods described in this section, you can use the sample files
from the Fluorescent Genotyping Demonstration Kit. The Tutorial disk supplied with the
installation disks for Genotyper 2.0 software contains the data files.
8-12 Microsatellite Analysis
Using the Histogram
To bin alleles using the Histogram window:
Window
Step
1
Action
Define the bin size as follows:
a.
From the Analysis menu, choose Set Statistics Options…
b.
Select the following buttons as shown below:
– Plot selection
– Size in bp
– Starting bin: determined automatically
c.
Enter 0.10 in the Bin size field.
Note
A bin size of 0.1 bp gives the most precise allele binning. If insufficient
data is available, however, the Genotyper software displays an error message
stating that the bin size is too small. If this occurs, increase the bin size.
2
From the View menu, choose Show Categories Window (or type K).
Microsatellite Analysis 8-13
To bin alleles using the Histogram window:
Step
3
(continued)
Action
Follow these steps to set up a Category (Group) for each marker.
a.
From the Analysis menu, choose Clear Category List.
b.
From the Category menu, choose Add Category.
c.
Enter the marker name, size range, and dye color for the first marker as shown
below.
d.
Click OK.
e.
Repeat these steps for the remaining markers:
– From the Category menu, choose Add Category.
– Enter the marker name, size range, and dye color.
– Click OK.
8-14 Microsatellite Analysis
4
From the Analysis menu, choose Label Peaks… Label peaks with Size in bp only.
5
From the Analysis menu, choose Filter Labels… Filter labels using the default
settings (best for dinucleotide repeat markers).
To bin alleles using the Histogram window:
Step
6
(continued)
Action
Working with one dye color at a time in the Main window:
a.
Click B to choose all blue dye/lanes.
b.
Draw a box in the plot window that covers all of the peaks associated with a
single marker.
c.
From the Views menu, choose Show Histogram Window.
d.
Make sure the correct marker name is displayed in the Category field. Leave
the Member field blank.
Note
All labeled peaks in the selected range for a given marker display as
vertical bars in the Histogram window. Each bar represents a particular size (x-axis,
value). The height represents the number of labeled peaks found for that size
(y-axis, counts). If you place the cursor on a particular peak/bar, Genotyper
software displays the corresponding value and counts.
7
Draw a box around a bar or group of bars that represent one allele. The area inside
the box is the allelic bin. Genotyper software displays the size range for the bin and
the number of peaks found in that range in the status box at the bottom of the
window.
Microsatellite Analysis 8-15
To bin alleles using the Histogram window:
Step
8
(continued)
Action
From the Category menu, choose Add Category…
Genotyper software automatically:
♦
Enters the allele (member) set name to the rounded size in bp
♦
Enters the “Member of group” name (i.e., the marker name)
♦
Selects the Highest peak button
♦
Enters the allele size range (from x to y bp)
♦
Selects the dye color
♦
Selects the Exclusive checkbox
Note
Check the information entered automatically for accuracy.
Note
Genotyper software will not allow the addition of a new group if a group or
category with the same name already exists.
9
Click OK to create a category member (allele bin) such as the one shown here.
10
Optional The bin shown in Step 9 was created with the size as a range. You can
also create a bin centered around the median size of the range with a set tolerance
(for example, 104.68 ± 0.5 bp) as follows:
a.
Hold down the Shift key while choosing Add Category… from the Category
menu.
b.
Edit the bin tolerance as desired. The size is displayed in the dialog box as
shown here.
Note
8-16 Microsatellite Analysis
The category member generated appears as follows:
To bin alleles using the Histogram window:
Step
11
(continued)
Action
Repeat these steps to continue adding categories for each allele. Remember to:
♦
Select the markers by color
♦
Verify that the Histogram window displays the correct marker name
Using the Plot
To bin alleles directly using the individual allele plots:
Window
Step
Action
1
From the Views menu, choose Show Categories Window (or type K) and set up
the main categories (Groups) for each marker as shown here.
2
From the Analysis menu, choose Label Peaks… Label peaks with Size in bp only.
3
From the Analysis menu, choose Filter Labels… Filter labels using the default
settings (best for dinucleotide repeat markers).
4
In the Main window, working with one dye color at a time:
5
a.
Choose all blue dye/lanes by clicking on the Blue color button to the left of the
dye/lanes window.
b.
Draw a box in the plot window that covers all of the peaks associated with a
single marker.
c.
From the Views menu, choose Zoom In (Selected Range), or type R, to
display the plots for the individual alleles.
Draw a box around the first tall peak from the left.
Microsatellite Analysis 8-17
To bin alleles directly using the individual allele plots:
Step
6
(continued)
Action
From the Category menu, choose Add Category… Genotyper software
automatically enters the size information for the category definition.
Enter the following information:
♦
Name of the allele (member) set to the rounded size in bp
♦
Member of group name (marker name)
♦
Highest peak button
♦
Size range of the allele (from x to y bp)
♦
Color of dye
♦
Exclusive checkbox
Note
You cannot add a new group if a group or category with the same name
already exists.
7
Click OK to add the category (bin).
8
Continuing to move from left to right, repeat step 4 through step 6 for the remaining
peaks.
9
Optional To create a bin centered around the median size of the range with a set
tolerance (for example, 104.68 ± 0.5 bp), follow these steps:
a.
Hold down the Shift key while choosing Add Category… from the Category
menu.
b.
Edit the bin tolerance as desired. The size is displayed in the dialog box as
shown here.
Binning Alleles You can use the Make from Labels… feature in Genotyper 2.0 software to generate
Using the Make from category members (allele bins) automatically. This method is ideal for the following
Labels… Feature types of linkage mapping/ genotyping projects:
♦
A single family/pedigree typed with a number of markers
♦
Small studies in which all markers for all individuals fit on a single gel
Unlike the other binning methods presented in this manual, using this method
requires:
♦
Working with one marker at a time to make categories from labels
♦
Clearing all labels between markers/categories
To bin alleles using the Make from Labels… feature:
Step
1
8-18 Microsatellite Analysis
Action
From the Views menu, choose Show Categories Window ( K) and set up the main
categories (groups) for your markers as follows:
To bin alleles using the Make from Labels… feature:
Step
(continued)
Action
2
From the Edit menu, choose Select All ( A) to select all categories.
3
From the Edit menu, choose Unmark ( U) to unmark the categories.
4
Select the first category in the list. From the Edit menu, choose Mark ( M).
5
If the first category…
Then…
is currently being defined
proceed directly to step 6.
is defined already
from the Analysis menu, choose Clear
All Labels.
6
Select the appropriate dye/lanes by clicking on the appropriate color button.
7
From the Analysis menu, choose Label Peaks… Label peaks with Size in bp only.
8
From the Analysis menu, choose Filter Labels… Filter labels using the default
settings (best for dinucleotide repeat markers).
9
From the Category menu, choose Make from Labels… to display the Make
Categories from Labels dialog box. Set the parameters as follows:
a.
Select Unmark overlapping categories and deselect Skip overlapping
categories.
To enable you to correct for overlaps, Genotyper software automatically
unmarks two or more category members that overlap in size based on the
tolerance.
b.
In the Name box:
– Either leave the Prefix field blank (Figure 8-1 on page 8-20) or enter a name
for the allele in the Prefix field (Figure 8-3 on page 8-21) which will become
part of the name of the alleles (Figure 8-2 on page 8-20 and Figure 8-4 on
page 8-21).
– In the First number box, enter the number of the first allele (the smallest allele
expected in the data, for example, 101) for the marker, or the starting number
(for example, 1) if using a prefix.
– In the Number increment box, enter a numeric value. This is the value by
which software automatically increases each successive allele number. For
example, enter 2 for dinucleotide markers if alleles are expected every 2 bp.
Enter 1 to number alleles sequentially (for example, A1, A2, A3, etc.).
10
c.
Select the With checkbox and the group name button.
d.
Enter the group/marker name in the field to the right of the group name
parameter. This indicates that the category members created belong to the
group/marker that you are currently working with.
e.
The appropriate dye color box should have been selected automatically by
Genotyper software. If not, check the appropriate box.
f.
Select the Exclusive checkbox if not automatically selected.
g.
Click OK.
Return to step 3 to define the remaining categories.
Microsatellite Analysis 8-19
To bin alleles using the Make from Labels… feature:
Step
(continued)
Action
11
When all the categories (markers) have been defined, choose Select All from the
Edit menu ( A) to select all categories. From the Edit menu, choose Mark ( M) to
mark all the categories.
12
From the Analysis menu, choose Clear All Labels. You can now label the alleles
with the newly defined bin names.
Figure 8-1 The Make from Labels…dialog box configured to use allele sizes as allele names
Figure 8-2 Example of allele bin names generated from the Make from Labels…dialog box
configured as shown in Figure 8-1
8-20 Microsatellite Analysis
Figure 8-3 The Make from Labels…dialog box configured to use a prefix for the allele name
Figure 8-4 Example of allelic bin names generated from the Make from Labels…dialog box
configured as shown in Figure 8-3
Using the Add You can use the Add Multiple Categories… feature to create a defined set of category
Multiple members (allele bins) that are equally spaced with a fixed tolerance.
Categories…
Once Genotyper software creates the categories, you can:
Feature
♦
Label and filter peaks
♦
Use the Histogram window to fine tune the category definitions
To define a set of equally spaced allelic bins with a fixed tolerance:
Step
1
Action
Set up the main categories (groups) for your markers as follows:
Microsatellite Analysis 8-21
To define a set of equally spaced allelic bins with a fixed tolerance:
Step
8-22 Microsatellite Analysis
(continued)
Action
2
From the Category menu, choose Add Multiple Categories… Choose the
appropriate settings for the first marker as follows:
3
Click OK to generate a set of categories for the marker as follows:
4
Repeat step 2 and step 3 for the rest of the markers making sure to enter the
appropriate starting size, dye color, and marker name in the Add Multiple
Categories dialog box.
5
From the Analysis menu, choose Label Peaks… Label peaks with Size in bp only.
6
From the Analysis menu, choose Filter Labels… Filter labels using the default
settings (best for dinucleotide repeat markers).
To fine tune the category definitions using the Histogram window:
Step
1
Action
Define the bin size as follows:
a.
From the Analysis menu, choose Set Statistics Options…
b.
Select the following buttons as shown below:
– Plot selection
– Size in bp
– Starting bin: determined automatically
c.
Enter 0.10 in the Bin size field.
Note
A bin size of 0.1 bp gives the most precise allele binning. If insufficient
data is available, however, Genotyper software displays an error message stating
that the bin size is too small. If this occurs, increase the bin size.
2
Click B to choose all blue dye/lanes.
3
In the Plot window, draw a box around all the peaks associated with a single
marker.
4
From the Views menu, choose Show Histogram Window.
Microsatellite Analysis 8-23
To fine tune the category definitions using the Histogram window:
Step
5
Action
Check the marker name displayed by the Category pop-up menu. If incorrect, select
the correct marker from the Category pop-up menu.
Note
8-24 Microsatellite Analysis
(continued)
Leave the Member pop-up field blank.
6
Select the Member pop-up menu to see a list of all the defined allele bins (category
members). The boundaries for each bin are displayed as vertical dotted lines in the
histogram. All the peaks/alleles belonging to a particular bin should fall between the
two outer boundaries of that bin. If they do not, proceed to the next step to adjust
the bin size.
7
From the Member pop-up menu, and choose the name of the bin you want to
adjust. Two “handles” are displayed on the corresponding bin boundaries.
8
Move the cross-hair cursor onto one of the handles until the cursor becomes a
cross-hairs in a circle. Click and drag the handle in or out as appropriate to redefine
the bin. Genotyper software automatically updates the bin size (category definition)
as you move the handles.
Troubleshooting Microsatellite Analysis
Common Problems The most commonly encountered problems during microsatellite analysis are:
♦
Poor or non-specific amplification
See Chapter 6, “Optimizing PCR,” and “Troubleshooting PCR Amplification” on
page 11-1 for suggestions.
♦
Incomplete 3´ A nucleotide addition
See page 6-18 for a discussion of the “plus-A” phenomenon and for suggestions.
♦
Stutter
See page 6-21 for a discussion of the stutter phenomenon and for suggestions.
See below for examples of stutter patterns in dinucleotide repeat loci.
Examples of
Stutter—
Dinucleotide
Repeats
Successful amplification of dinucleotide repeat markers yields allele peaks and
associated PCR stutter bands within a maximum range of eight base pairs from the
allele peak. The number of allele peaks depends on whether the individual tested is a
heterozygote or homozygote.
Dinucleotide repeats give specific stutter patterns that are illustrated in Figure 8-5
through Figure 8-9 on pages 8-25 through 8-27.
Example 1
The GeneScan electropherogram of a dinucleotide repeat marker from a homozygous
individual (118.6 bp, 118.6 bp) is shown in Figure 8-5.
The peaks at 116.6 bp, 114.6 bp and 112.6 bp are the typical 2-bp stutter pattern
seen with dinucleotide repeats. They represent the –2 bp, –4 bp, and –6 bp stutters
from the true 118.6-bp allele.
Figure 8-5 Typical pattern for dinucleotide repeat homozygote
Microsatellite Analysis 8-25
Example 2
The GeneScan electropherogram of a dinucleotide repeat marker from a
heterozygous individual (90 bp, 98 bp) is shown in Figure 8-6. Allele sizes differ by
8 bp.
The 2-bp stutter peak to the left of each allele peak is always of lower intensity than
the allele peak itself. The larger 98-bp allele peak is of lower intensity than the smaller
90-bp allele. In heterozygotes, the higher molecular weight allele often produces a
fluorescent signal of lower intensity than the lower molecular weight peak, suggesting
a less efficient amplification of the larger fragment.
Figure 8-6 Typical pattern for dinucleotide repeat heterozygote. Alleles differ by 8 bp.
Example 3
The GeneScan electropherogram from a dinucleotide repeat marker of a
heterozygous individual (86 bp, 90 bp) is shown in Figure 8-7 on page 8-26. Allele
sizes differ by 4 bp.
When the difference between the allele sizes is 4 bp or less, a shift occurs in the
height ratio between the two allele peaks (compare with Figure 8-6). The fluorescent
signal from the –4 bp stutter of the 90-bp allele is added to the signal from the 86-bp
allele.
Figure 8-7 Typical pattern for dinucleotide repeat heterozygote. Alleles differ by 4 bp.
Example 4
The GeneScan electropherogram from a dinucleotide repeat marker of a
heterozygous individual (92 bp, 94 bp) is shown in Figure 8-8. Allele sizes differ by
2 bp.
The fluorescent signal from the –2 bp stutter of the 94-bp allele is added to the signal
of the 92-bp allele. The signal from the –4 bp stutter band of the 94-bp allele is added
to the signal from the –2 bp stutter band of the 92-bp allele.
8-26 Microsatellite Analysis
A dinucleotide repeat marker for a heterozygous individual shows this typical triangle
pattern when the alleles differ by 2 bp.
Figure 8-8 Typical pattern for dinucleotide repeat heterozygote. Alleles differ by 2 bp.
Example 5
A GeneScan electropherogram for a dinucleotide repeat marker, displaying peaks at
1-bp intervals, is shown in Figure 8-9. AmpliTaq Gold and other DNA polymerases can
add a non-templated A to the end of a PCR product during amplification. When both
the true allele and allele-plus-A products show 2-bp stutter bands, a ladder of peaks
differing by 1 bp may be seen for PCR products. This phenomenon tends to be
locus-specific.
1
3
2
5
4
Figure 8-9 Typical pattern for dinucleotide repeat heterozygote showing 1-bp stutter. See
Table 8-2 for explanation of peak labels.
One allele in Figure 8-9 is labeled to indicate the origin of the peaks. The pattern
produced is a combination of both the 2-bp stutter peaks from the true allele and the
allele plus the non-templated A. The resulting peaks differ by 1 bp (Table 8-2).
Table 8-2 Origin of 1-bp peak pattern in dinucleotide repeat marker
Peak
Origin
1
+A product of allele peak
2
True allele peak based on DNA sequence
3
–2 bp stutter of +A peak
4
–2 bp stutter to true allele peak
5
–4 bp stutter of +A peak
continued on next page
Microsatellite Analysis 8-27
Is Stutter a Real Stutter, once understood, does not pose a real problem for microsatellite analysis. In
Problem? fact, stutter can actually aid in allele calling in two cases:
♦
Distinguishing true allele peaks from non-specific PCR products
Non-specific PCR products are not associated with stutter bands.
♦
Identifying alleles that fall far outside the reported allele range
The percent stutter is often specific to a particular locus. You can sometimes
identify alleles that fall far outside the previously reported range on the basis of
percent stutter.
8-28 Microsatellite Analysis
9
Microsatellite Analysis
Applications
9
Overview
In This Chapter This chapter provides instructions for performing specialized applications of
microsatellite analysis on the ABI PRISM® 310 Genetic Analyzer.
♦
Performing microsatellite analysis using the ABI PRISM™ Linkage Mapping Set
Version 2 (LMS V2)
♦
Screening for the loss of heterozygosity (LOH) of microsatellite markers linked to
known oncogenes or tumor-supressor genes
♦
Screening for evidence of replication error (RER) using microsatellite markers
♦
Determining animal paternity with the StockMarks® kits
♦
Determining human identity with the AmpFl STR™ kits
This chapter contains the following topics:
Topic
Microsatellite Analysis Using the LMS V2
See Page
9-2
Troubleshooting the LMS V2
9-4
LOH Screening
9-5
RER Screening
9-13
Troubleshooting LOH and RER Screening
9-16
Animal Paternity
9-17
Human Identification
9-19
Microsatellite Analysis Applications 9-1
Microsatellite Analysis Using the LMS V2
What is the The ABI PRISM Linkage Mapping Set Version 2 (LMS V2) contains 400 fluorescently
LMS V2? labeled PCR primers which amplify a highly informative subset of the microsatellite
loci from the Généthon human linkage map (Weissenbach et al., 1992; Gyapay et al.,
1994).
The LMS V2 consists of 28 panels, each containing 10–18 primer pairs. It expands the
capabilities of the original ABI PRISM Linkage Mapping Set with:
♦
New markers for improved resolution
♦
Tailed reverse primers for improved automatic allele calling
♦
A new dye set (containing NED) for improved spectral resolution of allele peaks
♦
True Allele™ PCR Premix (P/N 403061) with AmpliTaq Gold™ DNA Polymerase
This premix contains an optimized solution of AmpliTaq Gold DNA Polymerase,
dNTPs, and magnesium in a buffer for simpler, more reliable PCR amplification.
Advantages Product Performance and Quality Control
The primer pair combinations in all panels have been optimized for maximum
reliability. All have been tested on CEPH family 1347 and various sample DNAs to
confirm PCR conditions and to verify allele size ranges. In addition, Applied
Biosystems performs a final use test on all manufactured lots of primers using the
CEPH 1347-02 control DNA (P/N 403062).
New patented reverse-primer tailing (pig-tailing) chemistry improves allele calling
efficiency by eliminating problems associated with non-templated nucleotide addition.
ABI PRISM Technology
In addition to the high throughput afforded by the Applied Biosystems multicolor
fluorescence technology, the ABI PRISM 310 Genetic Analyzer allows extremely rapid
separations. Fragments that are 300 bp or less in length can be separated in under 30
minutes. This translates to a throughput of at least 48 samples in a 24-hour period.
The PCR conditions and optimized protocols described in this section were developed
using the following:
♦
GeneAmp® PCR System 9600
♦
True Allele PCR Premix with AmpliTaq Gold DNA Polymerase
♦
CEPH family 1347 DNA
When using other instruments, reagents, or DNA, some optimization might be
required.
continued on next page
9-2 Microsatellite Analysis Applications
Data Collection and Data collection and analysis are performed as for any microsatellite application. For
Analysis more information, refer to the ABI PRISM Linkage Mapping Set Version 2 User’s
Manual (P/N 904999).
Microsatellite Analysis Applications 9-3
Troubleshooting the LMS V2
If No Amplification For PCR failures, repeat PCR on the CEPH 1347-02 control DNA using the
Occurs recommended protocol in the ABI PRISM Linkage Mapping Set Version 2 User’s
Manual, Applied Biosystems reagents, consumables, and thermal cyclers. Make sure
that pipettes are calibrated, and that reagents have been stored properly.
If the control DNA is amplified, the problem may lie with the sample DNA. We suggest
you try the following:
♦
Use the PureGene DNA Isolation Kit (Gentra Systems, Inc., P/N D-5500A).
♦
Increase the pooling ratio of that marker.
♦
Perform a DNA titration with:
♦
–
1/5 less DNA than the original concentration
–
1/2 less DNA than the original concentration
–
Twice as much DNA as the original concentration
–
Five times as much DNA as the original concentration
Increase the number of PCR cycles from 30 to 33–35 by increasing the second
set of melt/anneal/extend cycles.
If amplification occurs using samples containing less DNA, inhibitors might be
present. Washing the samples in a Centricon-100 may help remove inhibitors.
If amplification occurs using samples containing more DNA, the original concentration
of DNA in the sample may not have been high enough, or the sample may be
degraded.
Optimizing Marker Increasing Signal Strength
Performance ♦ Increase the amount of a particular marker in your sample by adjusting the
pooling ratios for that marker.
♦
Increase the number of PCR cycles from 30 to 33–35 by increasing the second
set of melt/anneal/extend cycles.
♦
Increase the magnesium chloride concentration by performing a titration as
described on page 6-6. Background may increase as well.
♦
Decrease the annealing temperature 2–3 °C at a time. Background may increase.
Decreasing Background (Non-specific Amplification)
♦ Decrease the amount of the marker used by adjusting the pooling ratios if
background is interfering with allele calls of other markers.
♦
Increase the annealing temperature 2–3 °C at a time. Overall signal may
decrease.
9-4 Microsatellite Analysis Applications
LOH Screening
What is LOH? The body has many tumor-suppressing genes. These genes are functional unless one
or both of the alleles is lost or inactive, the remaining allele contains recessive
mutations, or both alleles contain recessive mutations. This allele loss is called loss of
heterozygosity (LOH). Analysis of DNA for LOH is a useful tool for the detection of
cancer.
The microsatellite markers used in LOH screening map either to known oncogenes or
to tumor-suppressor genes. Therefore, the loss of the DNA region containing the
linked oncogene or tumor-supressor gene often correlates both with the loss of LOH
markers and with the onset or susceptibility to certain types of cancer.
LOH is the second “hit” in the two-hit model. One needs to inherit a mutant oncogene
or tumor suppressor gene for LOH to cause cancer (Mulligan et al., 1990).
LOH screening has demonstrated reliability in the early detection of nonpolyposis
colon cancer, as well as for prognosis in confirmed cases (Aaltonen et al., 1993; de la
Chapelle and Peltomaki, 1995; Canzian et al., 1996). The application of this technique
to other tumor types only awaits further characterization of the relevant genes and
linked polymorphic markers.
Advantages The original LOH studies (Dryja et al., 1984; Mannens et al., 1988) employed DNA
probes that recognize RFLPs throughout the genome (Southern analysis).
PCR-based detection of LOH has the following advantages over Southern-based
LOH:
♦
It is faster than Southern-based detection of LOH.
♦
It requires only minute (nanogram) amounts of tumor DNA.
♦
It is suitable for formalin-fixed and paraffin-embedded archival tissue.
The third feature of PCR-based LOH will prove extremely useful in developing
tests to diagnose and predict the course of new types of cancer. Existing archival
tissue contains a wealth of genetic material along with complete patient histories.
Limitations ♦
Because LOH often appears in the same types of tumors as RER (replication
error, see page 9-13), in some instances you will need to perform LOH screening
in conjunction with RER screening. (The undetected presence of RER can mask
the presence of LOH, leading to a false-negative LOH diagnosis.)
♦
Extraction of high-quality DNA from formalin-fixed and paraffin-embedded tissue
can be difficult.
♦
If you cannot perform accurate DNA quantitation before PCR amplification,
interpretation of results can be difficult.
continued on next page
Microsatellite Analysis Applications 9-5
Advantages of Using In one study of cervical cancer, fluorescent detection had several key advantages over
ABI PRISM radioactive detection:
Technology ♦ Quantitative results were repeatable for a given locus.
♦
Results from contiguous loci were entirely consistent.
When two contiguous loci indicated LOH, the calculated LOH ratios were similar.
Rapid Screening
Analysis is rapid. Under ideal circumstances, you can analyze entire chromosomes at
a 20–30 cM resolution for 12 tumor/normal pairs in a single experiment. For any given
sample, you can detect LOH in 1 day.
The ABI PRISM 310 Genetic Analyzer allows extremely rapid separations. Fragments
that are 300 bp or less in length can be separated in under 30 minutes. This translates
to a throughput of at least 48 samples in a 24-hour period.
Microsatellite Any microsatellite markers can be used in LOH and replication error (RER) screening.
RER/LOH Assay Applied Biosystems offers two options:
♦
The Applied Biosystems Microsatellite RER/LOH Assay (P/N K0015) is a
fluorescent microsatellite assay that detects RER and loss of heterozygosity
(LOH) in genomic DNA isolated from microdissected normal and tumor tissue
pairs. This assay is for research purposes only. It can be used to help determine if
tumor cells are positive for the RER or the LOH phenotype.
The Microsatellite RER/LOH Assay includes reagents used for the polymerase
chain reaction (PCR) amplification of ten microsatellite markers located on several
chromosomes near known and suspected cancer genes. The assay also includes
control DNA.
Refer to the Microsatellite RER/LOH Assay User’s Manual (P/N L0089) for more
information.
♦
The ABI PRISM Linkage Mapping Set Version 2 (see page 9-2), a 10-cM
microsatellite map, has 400 markers that can also be used for LOH and RER
screening. However, this kit may require optimization for your application because
of the quantitative nature of LOH/RER screening.
9-6 Microsatellite Analysis Applications
Performing LOH Screening
Overview Microsatellites are amplified using one fluorescently labeled and one unlabeled primer
for each locus. Two amplifications are run for each microsatellite, one using sample
genomic DNA isolated from normal cells, and one using sample DNA isolated from
tumor cells from the same individual.
An GeneScan Internal Lane Size Standard is added to each sample before
denaturation and loading. The amplification products are separated and detected
using the ABI PRISM 310 Genetic Analyzer and the data is analyzed using GeneScan®
Analysis Software. Further analysis can be done using Genotyper® software.
Run Setup LOH run setup and operation is the same as for the basic microsatellite protocol given
in Chapter 8, with the following minor modifications:
♦
Run two DNA samples from each individual:
–
One from normal tissue (N)
–
One from tumor tissue (T)
Note
♦
Some normal tissue contaminating the tumor tissue sample is typical.
Run 3–4 independent injections for each sample (N and T).
This allows you to obtain sufficiently accurate quantitative estimates for
subsequent data analysis.
♦
In addition to the controls suggested for basic microsatellite analysis (see “Control
DNA” on page 8-5), obtain 8–10 confirmed N/T sample pairs to test the ability to
detect LOH.
Handling Samples Preventing Contamination
When using the PCR process, certain laboratory practices are necessary in order to
avoid false positive amplifications (Kwok and Higuchi, 1989). This is because the PCR
process is capable of amplifying single DNA molecules (Saiki et al., 1985; Mullis and
Faloona, 1987).
♦
Wear a clean lab coat (one never worn while handling amplified PCR products or
doing sample preparation) and clean gloves when preparing samples for PCR
amplification.
♦
Change gloves whenever contamination is possible.
♦
Maintain separate areas and dedicated equipment and supplies for:
–
Sample preparation
–
PCR setup
–
PCR amplification and analysis of PCR products
♦
Use aerosol-resistant (filter-plugged) PCR pipet tips.
♦
Never bring amplified PCR products into the PCR setup area.
♦
Open and close all sample tubes carefully. Try not to splash or spray PCR
samples.
♦
Keep reactions and components capped as much as possible.
♦
Clean lab benches and equipment regularly with 10% bleach solution.
Microsatellite Analysis Applications 9-7
Precautions for Working with Human Tissue
! WARNING ! BIOHAZARD. Tissue samples have the potential to transmit infectious
diseases. Follow the latest guidelines published by the Centers for Disease Control
(CDC) and National Institutes of Health (NIH) concerning the principles of risk
assessment, biological containment, and safe laboratory practices for activities
involving clinical specimens. These principles can be found in the U.S. Department of
Health and Human Services (HHS) publication, Biosafety in Microbiological and
Biomedical Laboratories (publication number 93-8395, stock number 017-040-523-7). The
biosafety Level 2 containment elements are consistent with the Occupational Health and
Safety Administration (OSHA) requirements contained in the HHS OSHA Bloodborne
Pathogen Standard 29 CFR, part 1910.1030.
Preparing DNA Extract DNA
Genomic DNA for the RER/LOH Assay can be extracted from fresh, frozen, or
paraffin-embedded tissue.
For successful results, particularly when extracting DNA from paraffin-embedded
tissue, you can use the following:
♦
Nucleon Genomic DNA Kit (Scotlab, P/N SL-8501)
♦
PureGene DNA Isolation Kit (Gentra Systems, Inc., P/N D-5500A)
♦
QIAamp Tissue Kit (Qiagen, Inc., P/N 29304)
Good yields of DNA have been obtained in Applied Biosystems laboratories using any
of these kits and have also found that they work well to eliminate PCR inhibitors from
the DNA. Extract the DNA as described in the protocol provided with these kits.
Note
The quality of genomic DNA isolated from paraffin-embedded tissue will vary with the
type of fixative used, the time in formalin, the age of the sample, and the method of DNA
isolation.
Evaluate DNA Quality and Quantity
After DNA extraction it is critical to evaluate DNA quantity. This can be done using the
QuantiBlot® Human DNA Quantitation Kit (P/N N808-0114) or spectrophotometrically
using Picogreen (Molecular Probes, P/N P-7581).
DNA quality and quantity can also be evaluated by electrophoresing 5 µL of genomic
DNA through a 1% Seakem GTG agarose gel with 0.8 µg/mL ethidium bromide.
Note
The genomic DNA must be quantitated accurately for the assay to be successful.
Estimate DNA yields by comparing the isolated DNA to DNA standards of known
molecular weight and concentration. A 5-µm section of 1 cm2 paraffin-embedded
tissue generally yields 100–500 ng of DNA. The size of the DNA typically ranges from
200 base pairs (bp) to one kilobase pair (kb) or more, depending on how the tissue
was processed.
continued on next page
9-8 Microsatellite Analysis Applications
PCR Amplification The protocols described here use the Microsatellite RER/LOH Assay, which is
optimized for LOH/RER assays and includes appropriate controls. This kit is a
convenient way to become familiar with these assays, even if your loci of interest are
not in the kit.
Preparing PCR Samples
This procedure describes how to prepare DNA samples for amplifying specific loci
within the human genome. Refer to the Microsatellite RER/LOH Assay User’s Manual
for more information.
Step
Action
1
Label ten (one for each marker) 0.2-mL MicroAmp® tubes for each control sample
and ten for each tumor sample.
2
Thaw and gently vortex the PCR Mix.
3
In an area free of PCR products, aliquot 15 µL of the PCR Mix into each MicroAmp
tube.
4
Dilute the DNA to a final concentration of 10 ng/µL using sterile-distilled water or
DNA Diluent Buffer.
Note
If 1X TE buffer is used to dilute genomic DNA, the EDTA in the buffer will
alter the magnesium concentration in the PCR Mix, and potentially influence the
amplification results.
5
Combine the following to prepare 60 µL of 12X Master Mix:
♦
DNA Diluent Buffer, 27.6 µL
♦
AmpliTaq Gold DNA Polymerase (5 U/µL), 2.4 µL
♦
Normal or tumor genomic DNA (10 ng/µL), 30 µL
6
Aliquot 5 µL of the Master Mix into each MicroAmp tube containing the PCR Mix.
7
Close the MicroAmp tubes.
8
Place the MicroAmp tray with samples into a centrifuge with a 96-well adapter. Spin
the tubes for 20 seconds at 150 × g.
9
Place the MicroAmp tray with samples into the thermal cycler.
10
Program the GeneAmp® PCR System 9600 as described in “Thermal Cycling” on
page 9-10.
Note
Upon completion of thermal cycling, you may store the samples at 2–6 °C.
Microsatellite Analysis Applications 9-9
Thermal Cycling
The thermal cycling conditions in Table 9-1 and Table 9-2 are optimized for the
GeneAmp 9600 PCR System. Other thermal cyclers may require reoptimization of
cycling conditions.
IMPORTANT
DNA from paraffin-embedded tissue requires more amplification cycles than
DNA from fresh or frozen tissue.
Table 9-1 Thermal Cycling Parameters for Samples Isolated from Fresh or Frozen Tissue
Step
Time
Temperature
AmpliTaq
Gold
Activation
PCR
Final
Extension
Preserve
Sample
Hold
30 Cycles
Hold
Hold
Denature
Anneal
Extend
10
minutes
10
seconds
30
seconds
3
minutes
30
minutes
Forever
95 °C
96 °C
55 °C
70 °C
70 °C
4 °C
Table 9-2 Thermal Cycling Parameters for DNA Samples Isolated from Paraffin-embedded Tissue
Step
Time
Temperature
AmpliTaq
Gold
Activation
PCR
Final
extension
Preserve
Sample
Hold
45 Cycles
Hold
Hold
Denature
Anneal
Extend
10
minutes
10
seconds
30
seconds
3
minutes
30
minutes
Forever
95 °C
96 °C
55 °C
70 °C
70 °C
4 °C
Pooling the Markers For specific information on pooling markers, refer to Chapter 2 of the ABI PRISM
Linkage Mapping Set Version 2 User’s Manual (P/N 904999).
Why Pool the Markers
It is necessary to pool markers in different volumes because:
♦
Primers amplifying markers are labeled with fluorescent dyes that vary in intensity.
♦
The yields of the PCR products from the few markers are different.
♦
DNA varies in amplification efficiency, especially DNA extracted from
paraffin-embedded tissue.
Optimizing Pooling Ratios
Occasionally one marker may amplify either more or less than expected. If the
fluorescent intensity is too high or too low:
♦
Load and run that one marker sample individually, or
♦
Adjust the pooling ratios
Note
Loading the gel with a volume of sample that gives a fluorescent signal of
approximately 500–1000 relative fluorescent units (RFU) will produce the most consistently
interpretable data. Although the dynamic range of the DNA sequencing instruments is
9-10 Microsatellite Analysis Applications
50–6000 RFU, a target of approximately 1000 RFU will ensure that data remains within this
range, even if there is slight sample-to-sample and run-to-run variation.
Analyzing Preliminary Data Analysis
LOH Data Follow the protocols for creating a matrix, setting Analysis Parameters, and analyzing
sample files provided in Chapter 8, “Microsatellite Analysis.”
For detailed instructions on using Genotyper to assess LOH see “Using Analyze and
Calculate in Table Commands—An LOH Example” on page 8-26 of the Genotyper
User’s Manual or Chapter 6 of the Microsatellite RER/LOH Assay User’s Manual.
Average Across Independent Injections
Once GeneScan software determines the peak height and area for all alleles of all
relevant microsatellite loci, use Genotyper software to pool the data from all the
independent injections of each N or T sample to obtain an average peak height and
area for every allele in every sample.
IMPORTANT
Do not combine N data with T data to obtain this average.
IMPORTANT
In almost any microdissection there are contaminating normal cells, so
normal DNA is present. Your results will depend upon the amount of contaminating normal DNA
in your sample.
Calculate the LOH Value
LOH can be defined mathematically as follows:
( height of normal allele two )
--------------------------------------------------------------------( height of normal allele one )
LOH = ---------------------------------------------------------------------(-----------------------------------------------------------------height of tumor allele two )( height of tumor allele one )
(Eq. 1)
An LOH value ≤0.5 indicates that the tumor sample shows significant loss of the
longer allele whereas an LOH value ≥1.5 indicates that the tumor sample shows
significant loss of the shorter allele.
Note
If a particular locus in an N sample is homozygous, you cannot use that locus to
diagnose LOH for the corresponding N-T pair.
Peak Height vs. Peak Area
Although a number of examples in the literature (e.g., Canzian et al., 1996; Cawkwell
et al.,1993) calculate LOH using peak area, we find peak height to be a more reliable
metric.
continued on next page
Microsatellite Analysis Applications 9-11
Sample Calculation Here is an example of a LOH calculation for the TP53-Penta marker, which is located
near the p53 gene.
Using Equation 1:
1343
-----------0.2073
1723
LOH = ------------ = ---------------- = 0.162
2315
1.283
-----------480
An LOH value of 0.16 clearly indicates loss of heterozygosity in the tumor sample.
In Figure 9-1, the first electropherogram corresponds to the normal tissue sample and
the second electropherogram to the tumor tissue sample. Peak heights are as shown
in Figure 9-1.
1723
1343
2315
480
Figure 9-1 Example of LOH at TP53-Penta
Preferential When alleles differ in size by ten or more base pairs you will likely observe preferential
Amplification amplification of shorter PCR products over longer ones (Walsh et al., 1992). This will
also occur when amplifying low copy number DNA or DNA isolated from paraffin
embedded tissues. Be aware that preferential amplification can make LOH
measurements less accurate.
Figure 9-2 shows an electropherogram example of preferential amplification of the
D5S346 marker. In both the normal (top panel) and tumor (bottom panel) samples, the
peak height of the larger 124-bp fragment is much less than that of the smaller 110-bp
fragment.
Figure 9-2 Example of preferential amplification of the shorter PCR product at D5S346
9-12 Microsatellite Analysis Applications
RER Screening
What is RER? Replication error (RER), also called microsatellite instability, describes the reduced
fidelity during the replication of repetitive DNA often occurring in tumor cells. RER
leads to the appearance of multiple alleles at microsatellite loci. It is thought to be
caused by strand slippage during DNA replication due to mutations in DNA mismatch
repair genes.
The technique for detecting RER involves comparing microsatellite alleles after PCR
amplification in normal and tumor samples from the same host. You calculate a raw
“RER score” using an algebraic formula that quantifies the relative strength of the
stutter bands in the two samples after normalizing for differences in PCR efficiency.
Advantages RER is a simple, inexpensive, and reliable tool for the analysis of tumors.
Limitations The RER phenotype can be variable, ranging from a simple increase in the strength of
the stutter bands to the presence of extra bands on top of variable strength stutter
bands.
Although the formula for determining the raw RER score partially corrects for
differences in the amplification efficiency of normal and tumor samples, extreme
discrepancies in amplification efficiency can lead to false-positive or false-negative
results. For example, if the amplification of the normal sample is unusually poor,
Genotyper might only recognize the relatively strong peaks corresponding to the main
alleles. In an efficiently-amplified tumor sample, both the main-allele peaks and the
stutter peaks would be recognized. In this hypothetical case, you would obtain a
false-positive determination of RER.
Because RER often appears in the same types of tumors as LOH, RER screening
should be performed in conjunction with LOH screening. A false-negative RER
diagnosis can be obtained in LOH-positive samples.
continued on next page
Microsatellite Analysis Applications 9-13
Advantages of Using Increasing Reliability of RER Results
ABI PRISM Traditional approaches using radioactivity are labor-intensive, time-consuming, and
Technology difficult to automate. For example, multiple exposures of films are often required and if
normal and tumor DNA do not amplify with equal efficiency, interpretation becomes
difficult. Moreover, automation is highly desirable to reduce the arbitrariness in
analysis encouraged by the variability of the RER phenotype.
Co-electrophoresis To Increase Throughput
One of the primary advantages of using multiple dyes in RER screening is valid for
any microsatellite application: you can increase throughput by co-loading multiple
different reactions covering many relevant microsatellite loci for a single individual in
one capillary injection. Co-loading allows you to screen hundreds of individuals in a
single day.
Rapid Screening
The ABI PRISM 310 Genetic Analyzer allows extremely rapid separations. Fragments
that are 300 bp or less in length can be separated in under 30 minutes. This translates
to a throughput of at least 48 samples in a 24-hour period.
Protocol RER screening uses the same protocols as LOH screening (see page 9-7).
Examples of RER This section presents two classic examples of RER. Refer to them when interpreting
your own data.
Figure 9-3 shows the electropherogram of the dinucleotide repeat marker D18S35
from a homozygous individual. The appearance of numerous extra alleles at lower
molecular weights in the tumor sample (bottom panel) indicates significant genomic
instability.
Figure 9-3 An example of RER for a homozygote allele at D18S35
Figure 9-4 on page 9-15 shows the electropherogram of two dinucleotide repeat
markers (NM23 and D5S346) from one individual, heterozygous in both alleles. The
appearance of numerous extra alleles at both higher and lower molecular weight in the
tumor (bottom panel) sample indicates significant genomic instability.
9-14 Microsatellite Analysis Applications
Figure 9-4 An example of RER for heterozygote alleles at markers NM23 and D5S346
RER is often more subtle than is shown in these examples. Virtually all difference
between normal and tumor samples that are not LOH are interpreted as replication
error. In general, you should see RER in more than one marker to be sure that it is
really genomic instability that you are observing and not merely an artifact.
Note
While both microsatellite instability and loss of heterozygosity are indicative of
cancerous tissue, if an electropherogram shows RER at a given marker location, an LOH
calculation for that allele region is complicated or even invalid (Canzian et al. 1996). We do not
recommend LOH calculations in regions that show clear signs of RER.
Microsatellite Analysis Applications 9-15
Troubleshooting LOH and RER Screening
Common LOH and Most problems in LOH and RER screening are common to all microsatellite
RER Problems applications. See Chapter 11 for more information. A few problems that are more
specific to LOH and RER screening are described in Table 9-3.
Table 9-3 Troubleshooting LOH and RER Screening
Observation
Possible Cause
Recommended Action
No bands on
GeneScan gel
PCR amplification failed due to
presence of PCR inhibitors.
Run DNA sample on an agarose
gel.
If DNA is present, repurify the
sample using the QIAamp Tissue
Kit or other commercial kit to
remove PCR inhibitors.
DNA degraded.
Incorrect DNA loading or
mispipetting.
Preferential
amplification of
shorter PCR
products over longer
ones
9-16 Microsatellite Analysis Applications
Alleles are separated by ten
base pairs or more.
If no DNA is observed on an
agarose gel, prepare new DNA
from the tissue sample.
Make sure the DNA is
quantitated accurately for both
the normal (N) and tumor (T)
samples.
Animal Paternity
StockMarks Kits The StockMarks for Cattle® Bovine Paternity PCR Typing Kit uses 11 microsatellite
loci to automate the genotyping of cattle for breeding purposes.The StockMarks® for
Horses Equine Paternity PCR Typing Kit uses 12 microsatellite loci to automate the
genotyping of horses for breeding purposes.
Improved Breeding Humans have been breeding cattle and horses selectively for centuries. Animals that
exhibit superior production traits, such as high milk production, lean carcasses, speed,
or strength are used as breeding stock for subsequent generations. This classical
method requires the measurement of quantitative production traits and maintenance
of ancestral records by the breeding and racing associations. Recently, researchers
have turned to microsatellite markers to identify genetically desirable animals much
more quickly, reliably, and inexpensively.
The StockMarks kits have been used to perform the following:
♦
Parental identification for accurate pedigree analysis
♦
Quantitative trait loci (QTL) research to find markers linked to desirable traits
Advantages of The amplification capability of PCR, combined with the information content of
DNA-based Tests microsatellites, provides the following advantages:
♦
PCR-based tests are easy to standardize and automate, ensuring reproducible
results.
♦
PCR-based tests can be run on a variety of samples, including blood, semen, and
hair. Obtaining samples from hair eliminates the expense of having a veterinarian
draw blood. In addition, hair is easier to transport than blood.
♦
Very little sample is required for a positive result, unlike traditional serological
(blood) assays.
♦
Quicker, more accurate parentage identification can be obtained from DNA
analysis than from serological testing.
♦
DNA analysis allows inclusion as well as exclusion. An animal can be identified
positively as the parent rather than merely being eliminated as a possibility.
Advantages of Using One of the primary advantages of using multiple dyes in StockMarks analysis is valid
ABI PRISM for any mapping or identification application: you can increase throughput by
Technology co-loading multiple different reactions covering all relevant microsatellite loci for a
single individual in one capillary injection. Co-loading allows you to genotype
hundreds of animals in a single day.
You can also automate genotyping by analyzing your results with GeneScan Analysis
and Genotyper software (Figure 9-5 on page 9-18).
continued on next page
Microsatellite Analysis Applications 9-17
Allele Frequencies StockMarks for Cattle
Allele frequency information is currently available for the Holstein dairy cattle breed.
Similar frequency information is being collected for Aberdeen Angus, Red Angus,
Simmental, Gelbvieh, Salers, and South Devon. To test non-Holstein breeds with the
StockMarks for Cattle kit, you will first need to genotype approximately 20 unrelated
animals to determine if the Holstein frequencies apply to the breed of interest.
StockMarks for Horses
Allele frequency information is currently available for a number of horse breeds
(Warmblood 1 and 2, Standardbred, Fjord, Friesian, Throroughbred, and Tennessee
Walkers).
Genotyping A Genotyper plot of GeneScan results from the equine control DNA is shown in
Example Figure 9-5. All 12 alleles amplified by the StockMarks for Horses Equine Paternity
PCR Typing Kit are plotted.
Figure 9-5 Genotyper plot of the equine control DNA
For More Refer to the StockMarks for Cattle Bovine Paternity PCR Typing Kit Protocol
Information (P/N 401917) and the StockMarks for Horses Equine Paternity PCR Typing Kit
Protocol (P/N 402828) for more information. You can also find information about
animal paternity testing on the Agriculture page of the Applied Biosystems Web site
(www.appliedbiosystems.com/techsupport).
9-18 Microsatellite Analysis Applications
Human Identification
Human Short tandem repeat (STR) markers, also referred to as microsatellites, are
Identification with polymorphic DNA loci that contain a repeated nucleotide sequence. The STR repeat
STRs unit can be from two to seven nucleotides in length. The number of nucleotides per
repeat unit is the same for a majority of repeats within an STR locus. The number of
repeat units at an STR locus may differ, so alleles of many different lengths are
possible. Polymorphic STR loci are therefore very useful for human identification
purposes (Edwards et al., 1992).
STR loci can be amplified using the polymerase chain reaction (PCR) process and the
PCR products are then analyzed by electrophoresis to separate the alleles according
to size. PCR-amplified STR alleles can be detected using various methods, such as
fluorescent dye labeling, silver staining, or fluorescent dye staining.
The analysis of short tandem repeat loci is an important complement to the lengthand sequence-based DNA typing systems already in use for human identification. A
majority of the STRs that have been evaluated by the forensic community are
composed of four-nucleotide repeat units (Frégeau and Fourney, 1993; Kimpton et al.,
1993; Urquhart et al., 1995).
Advantages of STR PCR-based STR analysis has the following advantages over conventional methods of
Analysis DNA analysis such as Restriction Fragment Length Polymorphism (RFLP):
♦
PCR-based tests are rapid, giving results in 24 hours or less.
♦
The small size of STR loci improves the chance of obtaining a result, particularly
for samples containing minute amounts of DNA and/or degraded DNA.
♦
The small size range of STR loci makes them ideal candidates for co-amplification
while keeping all amplified alleles smaller than 350 base pairs. Many STR loci can
therefore be typed from a single PCR.
♦
STR alleles have discrete sizes, allowing for simplified interpretation of results.
♦
The STR alleles can be combined to form an allelic ladder, which is used to
genotype individuals.
♦
PCR-based STR tests can be automated, increasing laboratory throughput while
decreasing analysts’ hands-on time.
continued on next page
Microsatellite Analysis Applications 9-19
Applied Biosystems Applied Biosystems fluorescent multicolor dye technology allows multiple loci,
Fluorescent Dye including loci that have alleles with overlapping size ranges, to be analyzed in a single
Technology gel lane or capillary injection. Alleles for overlapping loci are distinguished by labeling
locus-specific primers with different color dyes.
Because only one primer of each pair is labeled, the ABI PRISM® instruments detect
only one strand for each amplified DNA fragment. The detection of only one strand
eliminates doublets arising from the different mobilities of complementary strands that
are often observed when using gel staining detection methods.
Automated Sizing Amplified samples can be analyzed in a slab gel format or can be injected into a
and Genotyping capillary. An internal lane size standard is loaded with each sample to allow for
automatic sizing of the PCR products and to normalize differences in electrophoretic
mobility between gel lanes or injections (Ziegle et al., 1992). GeneScan software
automatically analyzes the collected data, which can then be imported into Genotyper
software for automatic genotyping of alleles.
High Throughput Laboratories can analyze hundreds of loci in a single day using four-dye fluorescent
labeling. This is a dramatic increase in productivity compared with gel staining
techniques, which visualize all PCR products in the same color, or with other systems
that are limited to one or two colors.
continued on next page
9-20 Microsatellite Analysis Applications
AmpFl STR Loci The AmpFl STR™ PCR Amplification Kits co-amplify the repeat regions of various
short tandem repeat loci (Table 9-4). In some kits, a segment of the X-Y homologous
gene amelogenin is also amplified. Amplifying a segment of the amelogenin gene with
a single primer pair can be used for gender identification because different length
products from the X and Y chromosomes are generated (Sullivan et al.,1993).
Table 9-4 AmpFl STR loci
Locus
Designation
Chromosome
Location
Common Sequence Motif
Size Range
(bp)a
Dye Label
D3S1358
3p
TCTA (TCTG)1-3 (TCTA)n
114–142
5-FAM
vWA
FGA
12p12-pter
TCTA (TCTG)3-4 (TCTA)n
157–197
5-FAM
4q28
(TTTC)3 TTTT TTCT (CTTT)n CTCC (TTCC)2
219–267
5-FAM
Amelogenin
X: p22.1–22.3
Y: p11.2
–
–
107
113
JOE
D8S1179b
8
(TCTR)nc
128–168
JOE
TH01
11p15.5
(AATG)n
169–189
JOE
D21S11
21
(TCTA)n (TCTG)n [(TCTA)3 TA (TCTA)3 TCA (TCTA)2
TCCA TA] (TCTA)n
189–243
JOE
TPOX
2p23–2per
(AATG)n
218–242
JOE
D18S51
18q21.3
(AGAA)n
273–341
JOE
CSF1PO
5q33.3–34
(AGAT)n
281–317
JOE
D5S818
5q21–31
(AGAT)n
135–171
NED
D13S317
13q22–31
(GATA)n
206–234
NED
D7S820
7q
(GATA)n
258–294
NED
a. The size range is the actual base pair size of sequenced alleles contained in the AmpFlSTR Allelic Ladders. The sizes in the table include
the 3´ A nucleotide addition.
b. In some literature references, this locus is designated as D6S502.
c. R can represent either an A or G nucleotide.
continued on next page
Microsatellite Analysis Applications 9-21
AmpFl STR Kits The following AmpFl STR kits are currently available from Applied Biosystems:
♦
AmpFl STR Blue™ PCR Amplification Kit (P/N 402800)
♦
AmpFl STR Green™ I PCR Amplification Kit (P/N 402902)
♦
AmpFl STR Profiler™ PCR Amplification Kit (P/N 403038)
♦
AmpFl STR Profiler Plus™ PCR Amplification Kit (P/N 4303326)
Each AmpFl STR kit contains preformulated AmpFl STR PCR Reaction Mix, blended
primer set, AmpliTaq Gold™ DNA Polymerase, control DNA of known genotype,
mineral oil, and AmpFl STR Allelic Ladders. The PCR license rights for forensic testing
and research use are also included in the kit.
The AmpFl STR loci contained in the AmpFl STR kits are shown in Table 9-5.
Table 9-5 Loci in the AmpFl STR Kits
Locus
AmpFl STR Blue
AmpFl STR Green I
AmpFl STR Profiler
AmpFl STR
Profiler Plus
D3S1358
X
X
X
vWA
X
X
X
FGA
X
X
X
X
X
Amelogenin
X
TH01
X
X
TPOX
X
X
CSF1PO
X
X
D8S1179
X
D21S11
X
D18S51
X
D5S818
X
X
D13S317
X
X
D7S820
X
X
continued on next page
9-22 Microsatellite Analysis Applications
Genotyping Using The AmpFl STR Allelic Ladders contain the most common alleles of the loci and are
the AmpFl STR used to genotype the analyzed samples. The AmpFl STR Allelic Ladders in the
Allelic Ladders AmpFl STR Profiler Plus PCR Amplification Kit are shown in Figure 9-6.
Figure 9-6 Genotyper plot of the AmpFl STR Allelic Ladders contained in the AmpFl STR
Profiler Plus PCR Amplification Kit
When interpreting AmpFl STR kit results, genotypes are assigned to sample alleles by
comparison of their sizes to those obtained for the known alleles in the AmpFl STR
Allelic Ladders. Genotypes, not sizes, are used for comparison of data between runs,
instruments, and laboratories. We strongly recommend that laboratories use the
AmpFl STR Allelic Ladders on each gel or set of capillary injections to convert the
allele sizes to genotypes. The main reasons for this approach are outlined below:
♦
The size values obtained for the same sample can differ between instrument
platforms (ABI PRISM 310 Genetic Analyzer versus ABI PRISM® 377 DNA
Sequencer) because of differences in the type and concentration of the
gel/polymer matrices and in electrophoresis conditions.
♦
Sizes may differ between protocols for the same instrument platform because of
differences in gel or polymer concentration, run temperature, gel or capillary
thickness, and well-to-read length.
♦
Slight procedural and reagent variations between gels or between capillaries
result in greater size variation than that found between samples on the same gel
or between samples injected in the same capillary.
The internal lane size standard is run with every sample and is used to normalize
lane-to-lane or injection-to-injection migration differences, thereby providing excellent
sizing precision within a gel or within a set of capillary injections. Size windows based
on the allelic ladder are used to assign allele designations and genotypes to the
samples. The genotyping of samples by comparison to the AmpFlSTR Allelic Ladder
Microsatellite Analysis Applications 9-23
can be automated using Genotyper 2.0 software and the custom AmpFl STR template
files.
Reliable Results The AmpFl STR kit reagents and protocols have been optimized to produce the quality
of results necessary for human identification applications. Primers have been
designed to give a high degree of target specificity, maximum 3´ A nucleotide addition,
and balance in intensity between loci labeled with the same color dye (Figure 9-7).
Component concentrations of the reagents combined for PCR amplification (including
PCR reaction mix, primer set, and enzyme), are set in the middle of a range of
concentrations that give acceptable performance. To increase the success of
obtaining a result in the presence of enzyme inhibitors, bovine serum albumin (BSA)
has been included in the AmpFl STR PCR Reaction Mix.
GeneAmp PCR Instrument times and temperatures have been developed to produce
specific amplification while providing the necessary degree of sensitivity. The
recommended range of input DNA is 1.0–2.5 ng. Furthermore, instrument detection
protocols have been optimized to provide reproducible results with excellent resolution
and precision in sizing alleles.
Each AmpFl STR Kit has been validated according to the Technical Working Group on
DNA Analysis Methods (TWGDAM) guidelines. Validation was performed by scientists
at Applied Biosystems in conjunction with forensic laboratories. These validation
studies demonstrate that the AmpFl STR kits can be used reliably with Applied
Biosystems instruments and software to analyze samples commonly encountered in
forensic casework.
D3S1358
Amelogenin D8S1179
vWA
FGA
D21S11
D18S51
D5S818
D13S317
D7S820
Figure 9-7 GeneScan electropherogram of AmpFl STR Profiler Plus alleles in AmpFl STR
Control DNA 9947A
continued on next page
9-24 Microsatellite Analysis Applications
Discrimination The Probability of Identity (PI) and Probability of Paternity Exclusion (PE) values have
Power been determined for each AmpFl STR kit and are shown in Table 9-6. Allele
frequencies for each population database are provided in the respective user’s
manuals. Existence of random association (linkage equilibrium) among all 12 loci was
established.
Table 9-6 Discrimination Power of the AmpFl STR Kits
African-American
AmpFl STR Kit
U.S. Caucasian
PI
PE
PI
PE
AmpFl STR Blue
0.00021
N/A
0.00020
N/A
AmpFl STR Green I
0.00058
N/A
0.0024
N/A
AmpFl STR Profiler
1.23 × 10-10
0.9996
2.79 × 10-10
0.9994
AmpFl STR Profiler Plus
1.48 ×
10-11
0.999989
1.04 ×
10-11
0.999982
For More Refer to the following manuals:
Information ♦ AmpFl STR Blue PCR Amplification Kit User’s Manual (P/N 402827)
♦
AmpFl STR Green I PCR Amplification Kit User’s Manual (P/N 402944)
♦
AmpFl STR Profiler PCR Amplification Kit User’s Manual (P/N 402945)
♦
AmpFl STR Profiler Plus PCR Amplification Kit User’s Manual (P/N 4303501)
These manuals contain sections describing the following:
♦
background information on the respective AmpFl STR kits
♦
guidelines for setting up a laboratory for PCR DNA analysis
♦
recommended protocols for DNA extraction
♦
the importance of DNA quantitation prior to STR analysis
♦
protocols for PCR amplification of the kit loci
♦
information on the multicomponent analysis of fluorescence data
♦
protocols for detection and analysis of PCR products
♦
guidelines for interpretation of results
♦
the use of Genotyper software for automated genotyping of alleles
♦
guidelines for troubleshooting results
♦
summaries of the validation work for the respective kits according to the
guidelines established by the Technical Working Group on DNA Analysis Methods
(TWGDAM)
♦
population genetics data for the kit loci
The sections detailing how to set up a laboratory for PCR DNA analysis and how to
perform the recommended protocols for DNA extraction can be used by all
laboratories that perform PCR analysis. These sections are updated from the Applied
BiosystemsAmpliType® User’s Guide (Versions 1 and 2).
Microsatellite Analysis Applications 9-25
AFLP Mapping
10
10
Introduction
What is AFLP? The AFLP™ amplified fragment polymorphism technique is used to visualize hundreds
of amplified DNA restriction fragments simultaneously. The AFLP band patterns, or
fingerprints, can be used for many purposes, such as monitoring the identity of an
isolate or the degree of similarity among isolates. Polymorphisms in band patterns
map to specific loci, allowing the individuals to be genotyped or differentiated based
on the alleles they carry.
AFLP technology combines the power of restriction fragment length polymorphism
(RFLP) with the flexibility of PCR-based technology by ligating primer-recognition
sequences (adaptors) to the restricted DNA.
Advantages of AFLP The advantages of the AFLP technique include the following:
♦
Only small amounts of DNA are needed.
♦
Unlike randomly amplified polymorphic DNAs (RAPDs) that use multiple, arbitrary
primers and lead to unreliable results, the AFLP technique uses only two primers
and gives reproducible results.
♦
Many restriction fragment subsets can be amplified by changing the nucleotide
extensions on the adaptor sequences. Hundreds of markers can be generated
reliably.
♦
High resolution is obtained because of the stringent PCR conditions.
♦
The AFLP technique works on a variety of genomic DNA samples.
♦
No prior knowledge of the genomic sequence is required.
Applications Applications for AFLP in microbial fingerprinting include:
of AFLP ♦ differentiation and tracking of highly related microbes at the species or strain level
♦
high-resolution genotyping for taxonomic applications
♦
detection of DNA polymorphisms in genome evolution studies
♦
determining the relatedness of pathogenic organisms in epidemiological studies
♦
mapping of cloned fragments in bacterial and yeast artificial chromosomes (BACs
and YACs)
An example of AFLP microbial fingerprints is shown in Figure 10-1 on page 10-2. The
first 24 lanes show six samples each of four different Escherichia coli strains (each of
the six samples represents a different growth phase of the organism). The final 11
AFLP Mapping 10-1
lanes show different growth phases of a single strain of Legionella pneumophila. Note
that the E. coli fingerprints are similar to each other and different from the Legionella
fingerprint. Within a strain, all of the bands are reproducible. Large population studies
provide data for the linkage of a band with a given phenotype, such as pathogenicity.
E. coli strains
Legionella strain
Figure 10-1 AFLP fingerprints of four E. coli strains and one Legionella strain
Applications for AFLP in plant mapping include:
♦
establishing linkage groups in crosses
♦
saturating regions of introgression with markers for gene landing efforts
♦
assessing the degree of relatedness or variability among cultivars
Examples of AFLP plant mapping are shown in Figure 10-2 and Figure 10-3 on
page 10-3 and Figure 10-4 on page 10-4.
10-2 AFLP Mapping
Figure 10-2 AFLP plant mapping gel. Note that the pattern is much more complicated for
plants than for bacteria.
You can build a genetic map of markers showing Mendelian inheritance from AFLP
data such as that shown in Figure 10-3. The four electropherogram panels in
Figure 10-3 contain data from tomato DNA samples prepared using the AFLP
technique. Samples were run on an ABI™ 373 DNA Sequencer and the resulting data
analyzed using GeneScan® Analysis Software.
P1, P2, F1
F2 (1)
F2 (2)
F2 (3)
Figure 10-3 Tomato AFLP samples showing Mendelian segregation
The overlapping electropherograms in the top panel are AFLP results of sample DNA
from three individuals: parent one (P1), parent two (P2), and F1 from a cross. A and B
are the two significant peaks on this panel and appear only in P2 and F1.
The lower three electropherogram panels are AFLP results of sample DNA from three
F2 generations. Peak A appears in F2 (3), but does not appear in either F2 (1), or F2
(2). Peak B is inherited in all three F2 individuals. The remaining non-polymorphic
AFLP Mapping 10-3
peaks appear in all three F2 electropherograms and show that the overall AFLP
patterns are reproducible.
Figure 10-4 Rice AFLP samples showing near-isogenic regions
The two electropherogram panels shown in Figure 10-4 contain data from rice DNA
samples prepared using the AFLP technique. Samples were run on an ABI 373 DNA
Sequencer and the resulting data analyzed using GeneScan Analysis Software.
The rice DNA was isolated from near-isogenic lines (almost identical genetic
material). It was selected for an introgressed region carrying a disease-resistance
gene. By comparing peak patterns in the two electropherograms, you will find that the
rice lines differ by only 1–2%. One of the peaks distinguishing the two lines has been
highlighted in both the electropherogram display and the related tabular data beneath
the electropherogram panels.
For examples of other applications, refer to the literature cited in Appendix D.
For More Refer to the AFLP Microbial Fingerprinting Protocol (P/N 402977) and the AFLP Plant
Information Mapping Protocol (P/N 4303146) for more information.
10-4 AFLP Mapping
The AFLP Technique
Template The first step of the AFLP technique is to generate restriction fragments by using two
Preparation and restriction endonucleases (EcoRI and MseI in the AFLP Microbial Fingerprinting and
Adaptor Ligation AFLP Plant Mapping Kits). Double-stranded adaptors supplied with each kit are
ligated to the ends of the DNA fragments, generating template DNA for subsequent
polymerase chain reaction (PCR) amplification.
Restriction and ligation may take place in a single reaction if the buffers are
compatible (Figure 10-5). Adaptor sequences have been designed such that ligation
of the adaptor oligonucleotide to the restricted DNA does not regenerate the
recognition site. If the buffers are not compatible, the reactions must be run
sequentially.
Figure 10-5 Example of template preparation and AFLP adaptor ligation
Preselective
Amplification—
Microbial
Fingerprinting
The sequences of the adaptors and the restriction site serve as primer binding sites
for a subsequent low-level selection or “preselective” amplification of the restriction
fragments.
Only those genomic fragments that have an adaptor on each end amplify
exponentially during PCR amplification (Figure 10-6). This step effectively “purifies”
the target away from sequences that amplify only linearly, i.e., those with one modified
end.
Figure 10-6 Preselective amplification of the prepared template
In the microbial genomes targeted by the AFLP Microbial Fingerprinting Kit
(P/N 402948), the core primer sequence is used. In larger genomes, such as plants
AFLP Mapping 10-5
and some fungi, this amplification would create too many fragments. In those cases,
the preselective amplification is performed with additional nucleotides on the end of
each primer (see page 10-7). Each added nucleotide reduces the number of
sequences by a factor of four.
The thermal cycling conditions of the preselective amplification step have been
optimized to generate a constant final mass of fragments. Band intensity in
subsequent reactions can therefore be correlated with relative differences in
representation of the fragments within the genome, and not to the overall amount of
genomic DNA that went into the initial restriction-ligation mix.
It is not necessary to perform this step if:
Selective
Amplification—
Microbial
Fingerprinting
♦
relative peak height information is not desired
♦
methods are available to normalize the final signal
♦
very accurate quantitation of the input DNA is performed routinely
Additional PCR amplifications are run to reduce the complexity of the mixture further
so that the fragments can be resolved on a polyacrylamide gel. These amplifications
use primers chosen from the 18 available AFLP Microbial Fingerprinting Kit Selective
Primers (nine EcoRI fluorescent dye-labeled primers and nine unlabeled MseI
primers). After PCR amplification with these primers, a portion of the samples is
analyzed on a Applied Biosystems DNA Sequencer.
Selective amplification with an EcoRI and an MseI primer amplifies primarily
EcoRI-MseI-ended fragments. The EcoRI-EcoRI fragments do not amplify well. The
MseI-MseI fragments are not visualized because they do not contain fluorescent dye
labels. Only the EcoRI-containing strands are detected (Figure 10-7).
Figure 10-7 Selective amplification with fluorescent dye-labeled primers
continued on next page
10-6 AFLP Mapping
Simplifying Figure 10-8 shows examples of AFLP fingerprint patterns that were prepared using
Complex Patterns different selective primers. Note that the EcoRI selective primers with one-nucleotide
extensions (EcoRI-A, EcoRI-T, and EcoRI-G) give simpler patterns than that obtained
using the primer with no extra nucleotide (EcoRI-0).
Figure 10-8 AFLP fingerprints of E. coli W3110 Reference DNA. The MseI-CA and
fluorescent dye-labeled EcoRI-0, EcoRI-A, EcoRI-T, and EcoRI-G selective primers (shown
here top to bottom, respectively) were used.
If the complexity of the AFLP pattern is still too high at the +2/+2 level, we recommend
reamplifying the preselective amplification sample with the preselective primers from
the AFLP Ligation and Preselective Amplification Modules of the AFLP Regular and
Small Plant Genome Mapping Kits (P/N 402004 and 402273, respectively).
Preselective The sequences of the adaptors and the restriction site serve as primer binding sites
Amplification— for a subsequent low-level selection or “preselective” amplification of the restriction
Plant Mapping fragments. The MseI complementary primer contains a 3´ C. The EcoRI
complementary primer contains a 3´ A (Regular Plant Genome Kit modules) or no
base addition (Small Plant Genome Kit modules).
Only those genomic fragments that have an adaptor on each end amplify
exponentially during PCR amplification (Figure 10-9 on page 10-8). This step
effectively “purifies” the target away from sequences that amplify only linearly, i.e.,
those with one modified end.
AFLP Mapping 10-7
Figure 10-9 Preselective amplification of the prepared template
Selective Additional PCR amplifications are run to further reduce the complexity of the mixture
Amplification— so that it can be resolved on a polyacrylamide gel. These amplifications use primers
Plant Mapping chosen from the 24 available AFLP Selective Primers (eight MseI and sixteen EcoRI
primers). After PCR amplification with these primers, a portion of each sample is
analyzed on a Applied Biosystems DNA Sequencer.
Selective amplification with an EcoRI and an MseI primer amplifies primarily
EcoRI-MseI-ended fragments. The EcoRI-EcoRI fragments do not amplify well. The
MseI-MseI fragments are not visualized because they do not contain fluorescent dye
labels. Only the EcoRI-containing strands are detected (Figure 10-10).
Figure 10-10 Selective amplification with fluorescent dye-labeled primers
Use the AFLP Selective Amplification Start-Up Modules (Regular Plant Genomes,
P/N 4303050; Small Plant Genomes, P/N 4303051) or individual AFLP Selective
Primers (see Table 10-3 on page 10-11).
continued on next page
10-8 AFLP Mapping
Testing New When testing novel genomes, you must be sure that the DNA restriction digest with
Genomes EcoRI and MseI generates enough fragments for comparison of samples. There is a
large variability in the number of restriction sites within microbial genomes. No
assurances of kit performance are made for organisms not listed.
Empirical guidelines suggest that if the G-C content of the genome is >65%, MseI will
not give a significant number of fragments. Optimal results are obtained with MseI
when the G-C content is <50%. EcoRI also tends to produce more fragments in
G-C-poor genomes. In cases where an organism’s G-C content is unknown, the
effectiveness of the restriction enzymes must be determined empirically.
Primer Selection
Guidelines—
Microbial
Fingerprinting
For genomes that restrict well with the EcoRI and MseI restriction endonuclease
combination, some general recommendations can be made in terms of the genome
size and the selective nucleotides to choose for subsequent amplification (Table 10-1).
Table 10-1 Guide to Choosing Selective Primers for Microbial Fingerprinting
Application
Nucleotide
Addition
EcoRI Primers
MseI Primers
Cosmids, BACs, P1
mapping
+0/+0
EcoRI-0 FAM
MseI-0
YACs, some larger
BACs
+0/+1
EcoRI-0 FAM
MseI-A
MseI-C
MseI-G
MseI-T
+1/+0
EcoRI-A FAM
EcoRI-C NED
EcoRI-G JOE
EcoRI-T JOE
MseI-0
+0/+2
EcoRI-0 FAM
MseI-CA
MseI-CC
MseI-CG
MseI-CT
+1/+1
EcoRI-A FAM
EcoRI-C NED
EcoRI-G JOE
EcoRI-T JOE
MseI-A
MseI-C
MseI-G
MseI-T
+2/+0
EcoRI-AA JOE
EcoRI-AC FAM
EcoRI-AG JOE
EcoRI-AT NED
MseI-0
Yeast, small fungi
genomes
+2/+2
EcoRI-AA JOE
EcoRI-AC FAM
EcoRI-AG JOE
EcoRI-AT NED
MseI-CA
MseI-CC
MseI-CG
MseI-CT
Large fungi genomes
+2/+3
+3/+2
Use the primers from the AFLP Regular and Small
Plant Genome Mapping Kits. See Table 10-3 on
page 10-11 for the primers available.
Bacteria
continued on next page
AFLP Mapping 10-9
Genome Analysis Some bacterial and fungal genomes that have been analyzed successfully using
Guide EcoRI, MseI, and the primers in the AFLP Microbial Fingerprinting Kit are shown in
Table 10-2.
Table 10-2 Genomes Analyzed with EcoRI and MseI Primer Pairs
Organism
Primer Pairs Used
Successfullya
Primer Pairs to Avoidb
Acinetobacter sp.
EcoRI-C/MseI-T
–
Aeromonas sp.
EcoRI-A/MseI-T
–
Aspergillus sp.
EcoRI-A/MseI-G
EcoRI-A/MseI-CA
EcoRI-C/MseI-CA
EcoRI-T/MseI-A
–
Bacillus sp.
EcoRI-0/MseI-A
–
Candida utilis
EcoRI-G/MseI-A
–
Clostridium sp.
EcoRI-C/MseI-C
–
Vancomycin-resistant
Enterobacter
EcoRI-A/MseI-T
EcoRI-G/MseI-A
EcoRI-T/MseI-C
–
Escherichia coli
EcoRI-0/MseI-C
EcoRI-A/MseI-C
EcoRI-G/MseI-A
EcoRI-T/MseI-C
EcoRI-0/MseI-A
EcoRI-0/MseI-G
Eutypa sp.
EcoRI-A/MseI-CA
EcoRI-AC/MseI-C
–
Legionella pneumophila
EcoRI-A/MseI-G
EcoRI-AC/MseI-C
EcoRI-0/MseI-A
Nensenula anomola
EcoRI-A/MseI-T
EcoRI-G/MseI-A
–
Paenibacillus larvae
EcoRI-C/MseI-A
–
Pichia membrefaciens
EcoRI-AC/MseI-C
Saccharomyces sp.
EcoRI-A/MseI-CA
EcoRI-AC/MseI-C
–
Schizosaccharomyces
pombe
EcoRI-AC/MseI-C
–
EcoRI-0/MseI-C
–
Xanthomonas sp.
a. Producing 25–130 bands evenly dispersed from 50–500 bases with intensities of
100–2000 relative fluorescent units
b. Too few or too many bands or uneven size distribution
Note
The list in Table 10-2 is not exhaustive. Refer to the publications listed in Appendix D
for in-depth discussion of primer choices.
continued on next page
10-10 AFLP Mapping
Primers Available— If you want to use a specific primer combination for the AFLP Selective Amplification
Plant Mapping reactions, you can order primer pairs in any combination of one EcoRI primer and one
MseI primer. This gives you 128 possible primer pair combinations from which you can
choose, for either regular or small plant genomes. Order the AFLP Amplification Core
Mix Module (P/N 402005) and the desired AFLP Selective Amplification Primers from
Table 10-3.
Table 10-3 AFLP Selective Amplification Primers for Plant Mapping
EcoRI Primers, Regular Plant Genomes
Primer
Part Number
(250 reactions)
Part Number
(500 reactions)
EcoRI-ACT FAM
402045
402037
EcoRI-ACA FAM
402038
402030
EcoRI-AAC NED
4303053
4303054
EcoRI-ACC NED
4303055
4303056
EcoRI-AGC NED
4303057
4303058
EcoRI-AAG JOE
402042
402034
EcoRI-AGG JOE
402043
402035
EcoRI-ACG JOE
402044
402036
EcoRI Primers, Small Plant Genomes
Primer
Part Number
(250 reactions)
EcoRI-TG FAM
402264
EcoRI-TC FAM
402265
EcoRI-AC FAM
402269
EcoRI-TT NED
4304352
EcoRI-AT NED
402955 (500 reactions)
EcoRI-TA JOE
402267
EcoRI-AG JOE
402268
EcoRI-AA JOE
402271
MseI Primers, Regular and Small Plant Genomes
Part Number
(250 reactions)
Part Number
(500 reactions)
MseI-CAA
402021
402029
MseI-CAC
402020
402028
MseI-CAG
402019
402027
MseI-CAT
402018
402026
MseI-CTA
402017
402025
MseI-CTC
402016
402024
MseI-CTG
402015
402023
MseI-CTT
402014
402022
Primer
continued on next page
AFLP Mapping 10-11
Plant Genomes Ten different crop species genomes were analyzed using the AFLP technique. For
Mapped Using each crop species, primer combinations that produce the best DNA fingerprints were
AFLP determined.
The names of each crop species tested and corresponding primer combination tables
are given in Table 10-4. Those combinations of EcoRI and MseI Selective
Amplification primers that are best suited for amplification screening of the designated
crop genomes are shown in Table 10-5 through Table 10-14.
Table 10-4 Primer Combination Tables for Crop Species
Crop Species
Primer Combination Table
Regular Plant Genomes
Sunflower
Table 10-5 on page 10-12
Pepper
Table 10-6 on page 10-13
Barley
Table 10-7 on page 10-13
Maize
Table 10-8 on page 10-14
Sugar beet
Table 10-9 on page 10-14
Tomato
Table 10-10 on page 10-15
Lettuce
Table 10-11 on page 10-15
Small Plant Genomes
Arabidopsis
Table 10-12 on page 10-16
Cucumber
Table 10-13 on page 10-16
Rice
Table 10-14 on page 10-17
following symbol indicates unacceptable primer combinations for
O The
amplification screening of designated species:
Table 10-5 Primer Combinations for Sunflower Species
MseI Primers
-CAA
EcoRI Primers
-ACA
-CAG
-CAT
-CTA
-CTC
O
-AAC
-AAG
-CAC
O
O
O
O O
-ACC
-ACG
O
O
-ACT
-AGC
-AGG
10-12 AFLP Mapping
O
O
-CTG
-CTT
Table 10-6 Primer Combinations for Pepper Species
MseI Primers
-CAA
-CAC
-CAT
-CTA
O O
O
O
-AAC
-AAG
EcoRI Primers
-CAG
-ACA
-CTC
-CTG
O
-CTT
O
O
-ACC
-ACG
-ACT
O
-AGC
O
-AGG
Table 10-7 Primer Combinations for Barley Species
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AAC
EcoRI Primers
-AAG
O O
-ACA
-ACC
-ACG
-ACT
-AGC
O
O
-AGG
AFLP Mapping 10-13
Table 10-8 Primer Combinations for Maize Species
MseI Primers
-CAA
-AAC
-CAC
-CAG
-CAT
EcoRI Primers
-CTC
-CTG
-CTT
O
O
O O
O
O
O
-AAG
-ACA
-CTA
O
-ACC
-ACG
O
-ACT
O
-AGC
-AGG
Table 10-9 Primer Combinations for Sugar Beet Species
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AAC
O
EcoRI Primers
-AAG
-ACA
-ACC
-ACG
-ACT
-AGC
-AGG
10-14 AFLP Mapping
O O
Table 10-10 Primer Combinations for Tomato Species
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AAC
O
EcoRI Primers
-AAG
O
-ACA
-ACC
-ACG
-ACT
-AGC
-AGG
Table 10-11 Primer Combinations for Lettuce Species
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AAC
EcoRI Primers
-AAG
O
O
-ACA
-ACC
-ACG
O
O
-ACT
-AGC
-AGG
O
AFLP Mapping 10-15
Table 10-12 Primer Combinations for Arabidopsis Species (Small Plant Genome)
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AA
EcoRI Primers
-AC
-AG
-AT
O
O
-TA
O
-TC
-TG
-TT
Table 10-13 Primer Combinations for Cucumber Species (Small Plant Genome)
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
O
-AA
EcoRI Primers
-AC
-AT
-TA
-TG
-TT
10-16 AFLP Mapping
O
-AG
-TC
-CTG
NOT DETERMINED
-CTT
Table 10-14 Primer Combinations for Rice Species (Small Plant Genome)
MseI Primers
-CAA
-CAC
-CAG
-CAT
-CTA
-CTC
-CTG
-CTT
-AA
EcoRI Primers
-AC
-AG
-AT
-TA
-TC
-TG
-TT
Fluorescent Applied Biosystems has adapted the AFLP technique for use with our ABI PRISM™
Dye-labeling and fluorescent dye-labeling and detection technology. PCR products are dye labeled
Marker Detection during amplification using a 5´ dye-labeled primer. For high throughput, you can
co-load up to three different reactions labeled with different colored dyes in a single
injection on the ABI PRISM® 310 Genetic Analyzer. Load a GeneScan Internal Lane
Size Standard in a fourth color in every lane or injection to size all amplification
fragments accurately.
You can automate the scoring of the large numbers of markers that are typically
generated by analyzing your results with GeneScan Analysis and Genotyper®
software.
AFLP Mapping 10-17
Troubleshooting
11
11
Troubleshooting PCR Amplification
Topics This section offers troubleshooting suggestions for the following problem areas:
♦
Problems with poor amplification (page 11-1)
♦
Problems with extra peaks (page 11-5)
♦
Problems with missing peaks (page 11-6)
Table 11-1 Problems with Poor Amplification
Observation
Possible Causes
Recommended Actions
Faint or no signal from
sample DNA and from
positive control
Insufficient enzyme in reactions
Use the recommended amount of
enzyme.
Incomplete activation of AmpliTaq Gold™ DNA
Polymerase
Repeat amplification, making sure to:
♦
Hold reactions initially at 95 °C for
10–15 minutes.
♦
Use the recommended buffer.
Note
Both buffer pH and buffer
composition affect enzyme activation.
Note
At temperatures >95 °C, the
enzyme is susceptible to irreversible
denaturation. If you suspect insufficient
activation, increase the incubation time,
not the incubation temperature.
Too little sample DNA added to reaction
Note
This is especially critical in human
identification experiments because sample
quality is often poor.
Quantitate DNA and use the amount
recommended in the protocol.
Note
For accurate quantitation of
human DNA samples, use the
QuantiBlot® Human DNA Quantitation
Kit (P/N N808-0114).
Troubleshooting 11-1
Table 11-1 Problems with Poor Amplification
(continued)
Observation
Possible Causes
Recommended Actions
Faint or no signal from
sample DNA and from
positive control
Incorrect or suboptimal thermal cycler
parameters
Check protocol for correct thermal cycler
parameters.
If the correct parameters were used,
they may need to be optimized for your
specific application. (For example allow
a linear increase in extension time with
increasing cycle number or increase
time at the denaturation plateau.)
PCR Master Mix not well mixed before
aliquoting
Vortex PCR Master Mix thoroughly.
Primer concentration too low
Use the recommended primer
concentration.
Primers degraded
Use new primers.
Note
Preincubation at 95 °C for 5–10
minutes should inactivate proteases or
nucleases.
Note
To prevent primer degradation
during storage, store primers at –15 to
–25 °C, either lyophilized or in TE. Avoid
excessive (more than 3–4) freeze-thaw
cycles.
Too little free Mg2+ in reaction
Check that you added sufficient total
Mg2+ given concentration of the dNTPs
and EDTA.
Note
[Free Mg2+] =
[Total Mg2+] – [Total dNTP] – 2[EDTA]
11-2 Troubleshooting
Incorrect pH
Verify buffer pH and buffer
concentration.
Wrong PCR tube
Use:
♦
Applied Biosystems GeneAmp®
Thin-Walled Reaction Tubes for the
DNA Thermal Cycler 480
♦
MicroAmp® Reaction Tubes with
Caps for the GeneAmp PCR
Systems 9600 and 2400
MicroAmp Base used with tray/retainer set and
tubes in GeneAmp® PCR System 9600 or
2400
Remove MicroAmp Base from
tray/retainer set and repeat
amplification.
Verify GeneAmp PCR System protocols and
programmed parameters
Refer to the thermal cycler user’s
manual and check instrument
calibration.
Tubes not seated tightly in the thermal cycler
during amplification (DNA Thermal Cycler 480)
Push reaction tubes firmly into contact
with block after first cycle. Repeat
amplification.
GeneAmp PCR System 9600 heated cover
misaligned
Align the heated cover so that white
stripes align after twisting the top portion
clockwise.
Table 11-1 Problems with Poor Amplification
(continued)
Observation
Possible Causes
Recommended Actions
Faint or no signal from
sample DNA and from
positive control
Poor thermal cycler performance
Check instrument calibration.
Good signal from positive
control but faint or no
signal from sample DNA
Sample contains PCR inhibitor (for example,
heme compounds, EDTA, or certain dyes)
Use a Applied Biosystems thermal
cycler.
Quantitate DNA. Dilute if possible in
order to add minimum necessary
volume. Repeat amplification.
Wash the sample in an Amicon
Centricon-100 column and repeat
amplification.
Note
For fragments smaller than
130 bp, use the Amicon Centricon-30
column instead.
Add bovine serum albumin (BSA) to the
PCR reaction mixture. (Use 8–16 µg
BSA for every 50 µL PCR reaction
volume.)
Sample DNA is degraded
Evaluate the quality and concentration of
the DNA sample by:
♦
Using the QuantiBlot Human DNA
Quantitation Kit (for human DNA)
♦
Running an agarose yield gel
If DNA is degraded or inaccurately
quantitated, reamplify with an increased
amount of DNA.
Insufficient sample DNA added because of
inaccurate quantitation
Evaluate the quality and concentration of
the DNA sample by:
♦
Using the QuantiBlot Human DNA
Quantitation Kit (for human DNA)
♦
Running an agarose yield gel
If DNA is degraded or inaccurately
quantitated, reamplify with an increased
amount of DNA.
Incorrect pH
Verify buffer pH and concentration.
If correct, quantitate sample DNA. Too
little or too much DNA can alter the pH.
Primer choice not optimal (for example,
primers may be annealing to sites of template
secondary structure or may have internal
secondary structure)
Use different primers.
Tm of primers is lower than expected
Decrease the annealing temperature by
2 °C increments.
See “Designing Custom Primers” on
page 6-3 for more information.
Troubleshooting 11-3
Table 11-1 Problems with Poor Amplification
(continued)
Observation
Possible Causes
Recommended Actions
Poor yield for multiplex
PCR
Non-optimal thermal cycling parameters
Between the denaturation and annealing
stages, add a 2 minute down-ramp time
to thermal cycling profile.
Note
For multiplex PCR, a short
down-ramp time is not necessarily
optimal.
Yield gets progressively
poorer for successive
PCR amplifications
performed over time
Competition from mispriming and other
competing side reactions
Use AmpliTaq Gold DNA Polymerase.
Problems with primer choice, concentration, or
degradation
See “Designing Custom Primers” on
page 6-3, “Determining Reagent
Concentrations” on page 6-6, and
“Multiplexing PCR” on page 6-10 for
additional suggestions.
Expired or mishandled reagents
Check expiration dates on all reagents.
See “Designing Custom Primers” on
page 6-3, “Multiplexing PCR” on
page 6-10, and “Preventing Competing
Side Reactions—Hot Start PCR” on
page 6-13 for additional suggestions.
If not expired, verify that reagents are
being stored and used according to
manufacturer’s instructions.
Compare with PCR performance using
fresh reagents.
Inconsistent yields with
control DNA
Combined reagents not spun to bottom of PCR
sample tube
Place all reagents in apex of tube and
spin briefly after combining.
Combined reagents left at room temperature
or on ice for extended periods of time
(encouraging mispriming and other primer
artifacts)
Put tubes in block immediately after
combining reagents.
Combined reagents not thoroughly mixed
Vortex all primers, reagents, and
reaction mixes (minus enzyme)
thoroughly to ensure uniform
concentration.
Primers not uniformly suspended before
adding to reaction mixture. (Primers can
aggregate and settle to the bottom of the tube.)
Pipetting errors.
Follow all these precautionary
measures:
♦
Calibrate pipettes
♦
Attach tips firmly
♦
Check all phases of pipetting
technique
♦
Whenever possible minimize
pipetting small volumes (for
example, make master mixes)
Note
You may also want to consider
using a 2-µL or other high-precision
pipette
continued on next page
11-4 Troubleshooting
Table 11-2 Problems with Extra Peaks
Observation
Possible Causes
Recommended Actions
Extra peaks appear with
no discernible pattern
Presence of exogenous DNA
Use appropriate techniques to avoid
introducing foreign DNA during
laboratory handling.
Nonspecific priming (i.e., primer-template
mismatch)
Check for good primer design. See
“Designing Custom Primers” on
page 6-3 for more information.
Add less template DNA.
Note
High DNA concentrations
promote nonspecific annealing.
Optimize Mg2+ concentration.
Add less primer DNA
Note
High primer concentrations
promote nonspecific annealing.
If you are not using AmpliTaq Gold DNA
Polymerase, consider using a Hot-Start
Technique.
Increase annealing temperature in
2–5 °C increments.
Decrease annealing and/or extension
times.
Increase primer length.
Perform a second amplification with
nested primers.
Perform Touchdown PCR.
Primer-dimer and primer-oligomer artifacts
(likelihood increases with multiplex PCR)
Check primers for 3´ complementarity.
Design longer primers.
Reduce primer concentration.
Reduce number of cycles.
Raise the annealing temperature in
2–5 °C increments.
Increase amount of target DNA.
Incomplete restriction (and/or ligation if
performing AFLP)
Repeat restriction (and/or ligation).
If performing AFLP, too much DNA in reaction
so that insufficient adaptor is present
Use the recommended amount of
template DNA.
Mixed sample
Verify quality and integrity of sample.
Troubleshooting 11-5
Table 11-2 Problems with Extra Peaks
(continued)
Observation
Possible Causes
Recommended Actions
Presence of split peaks
differing in size by one
base pair
Partial nontemplate addition of an extra
nucleotide (usually adenosine) to the blunt end
of the PCR product
Add the correct amount of Mg2+ to the
reaction mix.
(Extra peak of size n+1)
Note
Increasing Mg2+
concentrations can increase the
frequency of nontemplated nucleotide
addition and vice versa.
Increasing the extension time at 72 °C
will increase the frequency of
nontemplate nucleotide addition.
For more suggestions see “3´ A
Nucleotide Addition” on page 6-18.
Presence of peaks
differing in size by two,
three, or four base pairs
Stutter product formed during amplification of
di-, tri-, or tetranucleotide STR loci
See “Stutter Products” on page 6-21 for
suggestions.
(Extra peak of size n–2,
n–3, or n–4)
Table 11-3 Problems with Missing Peaks
Observation
Possible Causes
Recommended Actions
Some but not all loci
visible on
electropherogram
Sample DNA is degraded (indicated if shorter
amplicons are favored)
Quantitate DNA and add more template.
Repeat amplification.
Wash the sample in an Amicon
Centricon-100 column and repeat
amplification.
Note
For fragments smaller than
130 bp the Amicon Centricon-30 column
is preferable.
Individual alleles are
missing when inheritance
data is examined
11-6 Troubleshooting
Sample contains PCR inhibitor (e.g., heme
compounds, EDTA, or certain dyes)
Quantitate DNA and add minimum
necessary volume of PCR product.
Repeat amplification.
Mutation in primer annealing site of one allele
Change the primer.
Troubleshooting PCR Product Detection
Topics This section offers troubleshooting suggestions for the following problem areas:
♦
Problems with automatic data analysis (page 11-7)
♦
Problems with current (page 11-8)
♦
Problems with signal strength and quality (page 11-10)
♦
Problems with peak number and position (page 11-12)
♦
Problems with peak quality and resolution (page 11-14)
Table 11-4 Problems with Automatic Data Analysis
Observation
Possible Causes
Recommended Actions
Data was not
automatically analyzed
Sample Sheet not completed or completed
incorrectly
Complete the Sample Sheet as
described in your user’s manual.
Injection List not completed or completed
incorrectly
Complete the Injection List as described
in your user’s manual.
Analysis preferences set incorrectly in data
collection program
Check the collection software
preferences to make sure that
Autoanalyze with GeneScan® Analysis
Software is selected under the
GeneScan Injection List Defaults.
Insufficient free RAM
Restart the computer before collecting
data.
Note
You should always restart the
computer before collecting data.
Conflicting extensions
Choose Extensions Manager from the
Control Panels. Turn off any extensions
that were not part of the original
installation and restart computer.
continued on next page
Troubleshooting 11-7
Table 11-5 Problems with Current
Observation
No current
Possible Causes
Recommended Actions
Too little or no buffer in anode buffer reservoir
Replenish buffer reservoir.
Too little or no buffer in position 1 of
autosampler
Replenish buffer in position 1 of
autosampler.
Electrode bent
Replace or straighten electrode and
recalibrate autosampler.
Note
If you replace the electrode be
sure to clip it to the correct size.
Capillary bent away from electrode
Tape capillary securely to heat plate to
keep capillary from shifting position.
Place the tape on the heat plate just
above the electrode holder.
Refer to the ABI PRISM ® 310 Genetic
Analyzer User’s Manual.
Unfilled capillary or bubbles in capillary
Check system for leaks. Replace
capillary if necessary and rerun module.
Major leaks in system. Polymer does not enter
capillary
Check system for leaks.
Pump blockage (pump is plugged with urea or
crystallized buffer)
Remove and clean pump block. Refer to
the ABI PRISM 310 Genetic Analyzer
User’s Manual.
Loose valve fittings or syringe
Tighten valve fittings and syringe.
Anode buffer valve does not open
Open buffer valve.
Note
Filling the capillary should
cause the Gel Pump value in the Status
Window to increase by only 1–2 steps. If
the instrument detects a syringe leak, a
warning message appears on the
screen.
Note
The valve should depress
easily when you push the top with your
finger tip. After you release the pressure
the valve should spring to the “open”
position. If the valve is stuck, it should be
cleaned.
11-8 Troubleshooting
Plugged, broken, or nonconducting capillary
Replace the capillary.
Poor quality water in buffer solutions
Remake buffer with freshly autoclaved,
distilled, deionized water
Incorrect polymer solution formulation
Make or install new polymer solution
Corrupted firmware
Resend firmware by performing a cold
boot reset.
Syringe Pump Force too low. Capillary is not
being filled completely
Call DNA Technical Support.
Table 11-5 Problems with Current
(continued)
Observation
Possible Causes
Recommended Actions
Low current
Small bubble in capillary blocking current flow
Replenish gel in capillary.
Small bubble in pump block
Remove bubble by repriming the pump
block with polymer.
Plugged, broken, or nonconducting capillary
Replace the capillary.
Poor quality water in buffer solutions
Remake buffer with freshly autoclaved,
distilled, deionized water.
Old, defective, or incorrectly made buffer or
polymer solution
Replace buffer or polymer solution.
Too little buffer in anodic jar
Replenish buffer jar.
Fluctuating current
Small bubble in capillary blocking current flow
Replenish gel in capillary.
Small bubble in pump block
Remove bubble by repriming the pump
block with polymer.
Broken or cracked capillary
Replace the capillary.
Arcing to conductive surface on the instrument
Clean the hotplate and autosampler.
Ensure that the ambient temperature is
between 15 and 30 °C and the humidity
is below 80%. Check for excessive
condensation on the instrument.
Position of electrode is not sufficiently below
the buffer surface
Replenish buffer.
Current is normal at
beginning of run and then
decreases rapidly over
the next several minutes
Loss of anodic buffer capacity
Replace the buffer.
Current too high
Decomposition of urea in polymer solution
Add fresh polymer solution to the
syringe.
Incorrect buffer formulation (most likely too
concentrated)
Replace buffer with appropriate 1X
running buffer.
Arcing to conductive surface on the instrument
Clean the hotplate and autosampler.
Reposition electrode and recalibrate
autosampler.
Ensure that the ambient temperature is
between 15 and 30 °C and the humidity
is below 80%. Check for excessive
condensation on the instrument.
continued on next page
Troubleshooting 11-9
Table 11-6 Problems with Signal Strength and Quality
Observation
Possible Causes
Recommended Actions
No signal
No sample added
Add 1 µL PCR product to
formamide/size standard mix.
Sample not at bottom of tube
Spin sample tube in microcentrifuge.
Air bubble at bottom of sample tube
Spin sample tube in microcentrifuge to
remove air bubbles.
Capillary misaligned with electrode
Align capillary and electrode.
Note
The capillary should be
adjacent to, but not touching, the
electrode. The capillary should protrude
0.5 mm past the electrode.
Capillary bent out of sample tube
Align capillary and electrode.
Recalibrate autosampler.
Note
To verify whether a bent
capillary is the problem, watch the
movement of the autosampler tray
during run operation.
Autosampler not calibrated correctly
Calibrate autosampler in X, Y, and Z
directions.
IMPORTANT
The capillary should
almost touch the Z calibration point.
Sealed sample tube septum (i.e., septum will
not open to allow electrode into sample tube)
Replace septum.
Septum not placed in the sample tube properly
Signal too low
Insufficient sample added
Did you add a full 1 µL of PCR product
to formamide/size standard mix?
If no, add 1 µL PCR product to
formamide/size standard mix.
If yes, concentrate your PCR product
before adding to formamide/size
standard mix or examine the efficiency
of the PCR. Check pipette calibration.
11-10 Troubleshooting
Samples added to formamide that has
degraded to formic acid and formate ions
(leading to insufficient sample injected)
Use freshly deionized formamide. (See
“Deionized Formamide” on page A-3 for
directions.)
Ions in sample (leading to insufficient sample
injected)
Dialyze sample to remove ions.
Sample not thoroughly mixed with
formamide/size standard mixture
Mix sample into formamide/size
standard mixture by pipetting up and
down several times.
Insufficient [F]dNTPs added to PCR reaction
Reamplify using more [F]dNTPs or
examine the efficiency of the PCR.
Table 11-6 Problems with Signal Strength and Quality
Signal too high
(continued)
Too much sample injected into capillary.
Decrease injection time or injection
voltage.
Dilute sample before adding to
formamide/size standard mix.
Reamplify using less [F]dNTPs.
High baseline
Unincorporated [F]dNTPs
Purify the PCR product.
Dirty capillary window
Clean capillary window with 95%
ethanol.
Capillary moved out of position in front of laser
window
Position capillary in front of laser
window.
Precipitate in polymer
Allow polymer to equilibrate to room
temperature before using.
Use fresh polymer.
Noisy baseline
Spikes in baseline
Incorrectly prepared and/or old buffer or
polymer solutions
Replace buffer and polymer with fresh
solutions.
Fluorescing material in the capillary holder
Clean the capillary holder.
Defective capillary
Replace the capillary.
Matrix made incorrectly resulting in too much
correction (also indicated by troughs under
peaks)
Remake matrix. Be sure to:
Incorrectly prepared and/or old buffer or
polymer solutions
♦
Remove the primer peak (or
aberrant off-scale peaks) from the
scan range.
♦
Pick the start and stop points on flat
parts of the baseline when viewing
raw data.
♦
Make the matrix using same
polymer, buffer, and run conditions
as sample injections.
Replace buffer and polymer with fresh
solutions.
Dirty capillary holder aperture
Clean the capillary holder.
Defective capillary
Replace the capillary.
Precipitate in polymer
Allow polymer to equilibrate to room
temperature before adding to capillary.
Use fresh polymer.
Old polymer
Use fresh polymer.
continued on next page
Troubleshooting 11-11
Table 11-7 Problems with Peak Number and Position
Observation
Possible Causes
Recommended Actions
Extra peaks in additional
colors displayed
underneath the position
of one strong peak
Too much sample injected into capillary
(indicated if any peak is greater than
4000 RFU)
Decrease injection time or injection
voltage.
Dilute PCR sample before adding to
formamide/size standard mix.
Reamplify using less DNA.
Incorrect matrix chosen or poor matrix
Check matrix selection on Injection List.
If correct, create a new matrix.
Extra peaks when sample
is known to contain DNA
from a single source
Samples not fully denatured
Make sure the samples are heated at
95 °C for 5 minutes prior to loading onto
autosampler.
(If extra peaks are 1–4 nt
larger or smaller than
expected peak, it may be
a PCR artifact. See
“Problems with Extra
Peaks” on page 11-5.)
Unoptimized PCR
Check efficiency of the PCR. See
Chapter 6, “Optimizing PCR,” for
detailed suggestions.
Renaturation of denatured samples
Load samples immediately following
denaturation, or store on ice until you
are ready to load.
IMPORTANT
Do not store samples
on ice for more than 2 hours before
loading.
Note
Too much DNA also promotes
renaturation, but before you add less
DNA you will need to assess the signal
strength and quality.
Size standard peaks not
recognized when defining
size standard
Dust or dirt in polymer
Filter the polymer with a 0.2-µm or
0.4-µm disk filter attached to a plastic
syringe.
Height of a size standard peak less than the
Peak Amplitude Threshold for the size
standard color (in Analysis Parameters)
Rerun sample, adding the
recommended amount of size standard.
Note
11-12 Troubleshooting
50 RFU is the default threshold.
Peaks missing from size standard definition
Check GeneScan Analysis Parameters
to make sure the correct scan range is
defined.
Minimum Peak Half Width is set too high (in
Analysis Parameters)
Lower the value for the Minimum Peak
Half Width.
Table 11-7 Problems with Peak Number and Position
(continued)
Peak positions off
throughout size range
Incorrect Sample Sheet
Check Sample Sheet selection in data
collection program.
Note
See Chapter 5
for detailed information on
factors that affect sizing.
Change in size-calling method
Use consistent size-calling method.
Incorrect internal size standard
Use correct GeneScan Internal Lane
Size Standard.
Incorrect polymer composition
Check urea concentration and polymer
composition against protocol.
Incorrect electrophoresis temperature
Check the Injection List for temperature
setting.
If correct on Injection List, check the Log
for a recording of the actual
electrophoresis temperature.
Incorrectly defined size standard
Define size standard peak sizes
separately for each incorrectly sized
injection.
Inconsistent peak
mobilities at beginning of
run (i.e., peaks come off
at higher scan numbers in
the first injection)
Capillary temperature not at equilibrium
Repeat the injection of the first sample.
Runs get progressively
slower (i.e., size standard
peaks come off at higher
and higher scan
numbers)
Leaking syringe: polymer is not filling capillary
before every injection
Clean syringe thoroughly.
Syringe out of polymer
Fill syringe with fresh polymer.
Runs get progressively
faster (i.e., size standard
peaks come off at lower
and lower scan numbers)
Water in syringe
Prime syringe with small volume of
polymer, invert syringe to coat capillary
walls, and discard polymer.
Note
The run temperature can be set
in the Manual Control window while the
samples are being prepared, but we still
recommend repeating the first sample.
Replace syringe.
Then fill syringe with fresh running
polymer.
continued on next page
Troubleshooting 11-13
Table 11-8 Problems with Peak Resolution
Observation
Possible Causes
Recommended Actions
Poor resolution
Poor capillary performance
Replace capillary.
Incorrectly prepared and/or old buffer or
polymer solutions
Replace buffer and polymer with fresh
solutions.
Injection time too long (broad peaks)
Decrease injection time.
Incorrectly prepared and/or degraded sample
Prepare new sample.
Incorrect buffer formulation
Check if buffer formulation matches
protocol requirements.
Incorrect polymer composition
Check if polymer composition matches
protocol requirements.
Electro

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