TruSeq DNA Sample Prep Guide (15026486 C)

TruSeq DNA Sample Prep Guide (15026486 C)
TruSeq® DNA
Sample Preparation Guide
FOR RESEARCH USE ONLY
ILLUMINA PROPRIETARY
Part # 15026486 Rev. C
July 2012
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Part # 15026486 Rev. C
Revision History
Part #
Revision
Date
15026486
C
July
2012
15026486
B
April
2012
TruSeq DNA Sample Preparation Guide
Description of Change
• Added reagent volume table to Usage Guidelines
• Revised Tracking Tools documentation download information
• Removed detailed Sample Sheet description from Tracking Tools
• Added instructions for which assay to select when using the Illumina
Experiment Manager
• Updated Dual-Indexed Sequencing Platform Compatibility table
• TruSeq DNA Sample Prep v2 Kit renamed TruSeq DNA LT Sample Prep
Kit
• New TruSeq DNA HT Sample Prep Kit containing enough reagents for
96 samples and a DNA Adapter Plate (DAP). Information on the new
DAP is in included in the following sections:
• Usage Guidelines
• Indexed Adapter Sequences
• Adapter Options
• Pooling Guidelines
• Ligate Adapters procedures
• Enrich DNA Fragments procedures
• Low Throughput (LT) protocol renamed Low Sample (LS) protocol
• High Throughput (HT) protocol renamed High Sample (HS) protocol
• TruSeq DNA Sample Prep v2 documentation renamed TruSeq
DNA Sample Prep to encompass both the LT and HT kits and their
protocols
• Removed TruSeq DNA Sample Prep guide catalog number
• Guide content emphasizes the gel-free option is not used for
standard (whole-genome) sequencing and TruSeq Enrichment refers
to additional kits used for sequencing targeted regions
• Best Practices section changes:
• Renamed AMPure XP Handling to Handling Magnetic Beads
• Clarified Usage Guidelines
• Added Adapter Option, Pooling Guidelines (for low-plexity index
combinations), and Equipment sections
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iv
Part #
Revision
Date
15026486
B
(continued)
April
2012
Description of Change
• Tracking Tools section changes:
• Removed sample sheet format guidelines and direct reader to
sequencing analysis software user guide for detailed sample
sheet guidelines
• Illumina Experiment Manager introduced
• Added kit box A or B to Adapter Index Sequences table
• Kit Contents section changes:
• Corrected TruSeq DNA LT Sample Prep Kit catalog numbers
• Added number of indices to top level kit table
• TruSeq DNA LT Sample Prep Kit part numbers added
• PCR Primer Cocktail part number changed
• New TruSeq DNA HT Sample Prep Kit included
• User-Supplied Equipment section changes:
• Revised dark reader transilluminator catalog number
• Revised Magnetic stand-96 supplier to Life Technologies
• Updated recommended Covaris equipment with currently
available products and revised system settings in Fragment DNA
procedures
• Removed instructions throughout protocol to "take care not to
disturb the beads" and "change the tip after each sample", instead
adding a note in the introduction section of each protocol to
review the Best Practices on page 11
• Removed instructions throughout LS protocol to adjust pipette to
a specified volume before mixing.
• Removed steps in the procedures to pre-heat the thermal cycler lid
and thermal cycler program details, since thermal cycler
programming and lid heating instructions are provided in the
preparation section of each procedure
• Changed "multiplexed" to "indexed" throughout documentation to
refer to both dual-indexing and single-indexing
• Revised Ligate Adapters procedures to include the new DAP
component of the TruSeq DNA HT Sample Prep Kit
• Specified using the 12-well comb included with the recommended
gel system in Purify Ligation Products procedures
Part # 15026486 Rev. C
Revision
Date
B
(continued)
April
2012
15026486
A
August
2011
TruSeq DNA Sample Preparation Guide
Description of Change
• Enrich DNA Fragments:
• Removed "one tube each" following PMM and PPC specified in
preparation steps, since 1 tube per 48 reactions is required
• Named the thermal cycler program PCR
• Make PCR (LS protocol) - mixing step modified to adjust
pipette to 50 µl
• Clean Up PCR- AMPure XP Beads quantity differs if using
adapter index tubes or a DAP
• Make PDP - Updated pooling procedures to include 2–96 libraries
Initial Release
v
Revision History
Part #
15026486
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Part # 15026486 Rev. C
Table of Contents
Revision History
Table of Contents
List of Tables
Chapter 1 Overview
Introduction
Audience and Purpose
Chapter 2 Getting Started
Introduction
Acronyms
Best Practices
DNA Input Recommendations
In-Line Control DNA
Tracking Tools
Kit Contents
Consumables and Equipment
Indexed Adapter Sequences
Adapter Options
Pooling Guidelines
Chapter 3 Low Sample (LS) Protocol
Introduction
Sample Prep Workflow
Fragment DNA
Perform End Repair
Adenylate 3' Ends
Ligate Adapters
Purify Ligation Products (gel method only)
TruSeq DNA Sample Preparation Guide
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Enrich DNA Fragments
Validate Library
Normalize and Pool Libraries
Chapter 4 High Sample (HS) Protocol
Introduction
Sample Prep Workflow
Fragment DNA
Perform End Repair
Adenylate 3' Ends
Ligate Adapters
Purify Ligation Products (gel method only)
Enrich DNA Fragments
Validate Library
Normalize and Pool Libraries
Appendix A Alternate Fragmentation Protocols
Introduction
Procedure
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Index
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Technical Assistance
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Part # 15026486 Rev. C
List of Tables
Table 1 Protocol Features
Table 2 Kit and Sample Number Recommendations
Table 3 Kit and Protocol Recommendations
Table 4 Fragmentation Method Options
Table 5 TruSeq DNA Sample Preparation Acronyms
Table 6 TruSeq DNA Sample Prep Reagent Volumes
Table 7 In-Line Control Functions
Table 8 TruSeq DNA Sample Preparation Kits
Table 9 User-Supplied Consumables
Table 10 User-Supplied Consumables - Additional Items for LS Processing
Table 11 User-Supplied Consumables - Additional Items for HS Processing
Table 12 User-Supplied Equipment
Table 13 User-Supplied Equipment - Additional Items for HS Processing
Table 14 TruSeq DNA LT Sample Prep Kit Indexed Adapter Sequences
Table 15 TruSeq DNA HT Sample Prep Kit Indexed Adapter Sequences
Table 16 Dual-Indexed Sequencing Platform Compatibility
Table 17 Single-Indexed Pooling Strategies for 2–4 Samples
Table 18 Kit and Sample Number Recommendations
Table 19 Kit and Protocol Recommendations
Table 20 Fragmentation Method Options
Table 21 Covaris S220 or Covaris E220 Settings
Table 22 Covaris S2 or E210 Settings
Table 23 Size Selection Options
Table 24 Kit and Sample Number Recommendations
Table 25 Kit and Protocol Recommendations
Table 26 Fragmentation Method Options
Table 27 Covaris S220 or Covaris E220 Settings
Table 28 Covaris S2 or E210 Settings
Table 29 Size Selection Options
Table 30 Illumina General Contact Information
Table 31 Illumina Customer Support Telephone Numbers
TruSeq DNA Sample Preparation Guide
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Part # 15026486 Rev. C
Chapter 1 Overview
Introduction
Audience and Purpose
TruSeq DNA Sample Preparation Guide
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4
1
Chapter 1
Overview
Overview
Introduction
This protocol explains how to prepare up to 96 pooled indexed paired-end libraries of
genomic DNA (gDNA) for subsequent cluster generation and DNA sequencing using
the reagents provided in the Illumina® TruSeq® DNA Sample Preparation Kits (lowthroughput (LT) and high-throughput (HT)). The goal of this protocol is to add adapter
sequences onto the ends of DNA fragments to generate indexed single read or pairedend sequencing libraries.
The sample preparation protocol offers:
Streamlined Workflow
} Master-mixed reagents to reduce reagent containers and pipetting
} Universal adapter for preparation of single read, paired-end, and indexing
Gel-free option for TruSeq Enrichment with optimized AMPure XP bead conditions
Optimized shearing for whole-genome resequencing
Optimized workflows for processing low sample (LS) and high sample (HS) numbers in
parallel
Compatibility with low-throughput (LT) and high-throughput (HT) kit configurations
High Throughput
} Adapter plate allows for simultaneous preparation of 96 dual-indexed DNA
samples
} Volumes optimized for standard 96-well plate
Advanced Troubleshooting
} Process control checks built-in for quality control
Index Adapter Tags All Samples
} Additional adapters and primers not necessary
} Enables indexing earlier in the process
} The TruSeq DNA LT Sample Prep Kit contains adapter index tubes recommended
for preparing and pooling 24 or fewer samples for sequencing
} The TruSeq DNA HT Sample Prep Kit contains a 96-well plate with 96 uniquely
indexed adapter combinations designed for manual or automated preparation of 96
uniquely indexed samples
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Part # 15026486 Rev. C
Introduction
NOTE
• TruSeq Enrichment refers to the Illumina TruSeq Exome Enrichment and
TruSeq Custom Enrichment Kits that can be used following TruSeq DNA
Sample Prep to prepare the library for sequencing targeted regions. For
more information, see the TruSeq Enrichment Guide.
• The gel-free method is not an option when preparing libraries for
standard (whole-genome) sequencing.
The protocol is compatible with no indexing or a lower indexing pooling level. The
libraries generated do not require PCR amplification to enable cluster generation,
although PCR is recommended in the standard protocol to robustly meet the yield
requirements of most standard applications.
TruSeq DNA Sample Preparation Guide
3
Overview
Audience and Purpose
This guide documents the sample preparation protocol using the Illumina TruSeq DNA
LT Sample Prep Kit or TruSeq DNA HT Sample Prep Kit.
} Chapter 3 Low Sample (LS) Protocol explains how to perform the TruSeq DNA
Sample Preparation using the Low Sample (LS) Protocol
} Chapter 4 High Sample (HS) Protocol explains how to perform the TruSeq DNA
Sample Preparation using the High Sample (HS) Protocol
Equivalent results can be expected from either protocol and their distinguishing
elements are as follows:
Table 1 Protocol Features
LT Kit - Number of samples
processed at one time
HT Kit - Number of samples
processed at one time
Plate Type
Low Sample
≤ 48 with indexed
adapter tubes
High Sample
> 48 with indexed
adapter tubes
≤ 48 with indexed
adapter plate
> 48 with indexed
adapter plate
96-well 0.3 ml PCR
96-well MIDI
96-well HSP
96-well MIDI
96-well thermal cycler
Microheating system
Micro plate shaker
Incubation Equipment
96-well thermal cycler
Mixing Method
Pipetting
Illumina recommends the following kit, sample number, and protocol combinations:
Table 2 Kit and Sample Number Recommendations
4
Number of Samples
Processed
At One Time
Kit
Recommended
<24
LT
24–48
LT or HT
>48
HT
Part # 15026486 Rev. C
Audience and Purpose
Table 3 Kit and Protocol Recommendations
Kit
Number of
Samples
Supported
Number of Samples
Processed
At One Time
Protocol
LT
48
≤48
LS
>48
HS
≤48
LS
>48
HS
HT
96
The TruSeq DNA Sample Prep fragmentation process is optimized to obtain final
libraries, with the following differences
Table 4 Fragmentation Method Options
Whole-genome
Resequencing
Gel Method
Covaris
Shearing
Duration
Insert Size
40 seconds
300–400 bp
TruSeq Enrichment
Gel-free Method
Gel Method
120 seconds
100–900 bp
200–300 bp
NOTE
• TruSeq Enrichment refers to the Illumina TruSeq Exome Enrichment and
TruSeq Custom Enrichment Kits that can be used following TruSeq DNA
Sample Prep to prepare the library for sequencing targeted regions. For
more information, see the TruSeq Enrichment Guide.
• The gel-free method is not an option when preparing libraries for
standard (whole-genome) sequencing.
TruSeq DNA Sample Preparation Guide
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Part # 15026486 Rev. C
Chapter 2 Getting Started
Introduction
Acronyms
Best Practices
DNA Input Recommendations
In-Line Control DNA
Tracking Tools
Kit Contents
Consumables and Equipment
Indexed Adapter Sequences
Adapter Options
Pooling Guidelines
TruSeq DNA Sample Preparation Guide
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Chapter 2
Getting Started
Getting Started
Introduction
This chapter explains standard operating procedures and precautions for performing
TruSeq DNA Sample Preparation. You will also find lists of standard equipment and
consumables.
The sample preparation protocols described in the rest of this guide assume that you
are familiar with the contents of this chapter, have implemented all the
recommendations, and have obtained all of the requisite equipment and consumables.
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Part # 15026486 Rev. C
Acronyms
Acronyms
Table 5 TruSeq DNA Sample Preparation Acronyms
Acronym
Definition
ALP
Adapter Ligation Plate
ATL
A-Tailing Mix
CAP
Clean Up ALP Plate
CFP
Covaris Fragmentation Plate
CPP
Clean Up PCR Plate
CTA
A-Tailing Control
CTE
End Repair Control
CTL
Ligation Control
DAP
DNA Adapter Plate
DCT
Diluted Cluster Template
DNA
Customer Sample DNA Plate
dsDNA
double-stranded DNA
ERP
End Repair Mix
EUC
Experienced User Card
gDNA
genomic DNA
HSP
Hardshell Plate
HS
High Sample
HT
High Throughput
TruSeq DNA Sample Preparation Guide
9
Getting Started
Acronym
10
Definition
IMP
Insert Modification Plate
LIG
Ligation Mix
LS
Low Sample
LT
Low Throughput
LTF
Lab Tracking Form
PCR
Polymerase Chain Reaction
PDP
Pooled Dilution Plate
PMM
PCR Master Mix
PPC
PCR Primer Cocktail
RSB
Resuspension Buffer
SSP
Size Separate Plate
STL
Stop Ligation Buffer
TSP
Target Sample Plate
Part # 15026486 Rev. C
When preparing gDNA libraries for sequencing, you should always adhere to good
molecular biology practices. Read through the entire protocol prior to starting, to ensure
all of the required materials are available and your equipment is programmed and
ready to use.
NOTE
For more information, see the TruSeq Sample Preparation Best Practices and
Troubleshooting Guide which you can download from the Illumina website at
http://www.illumina.com. Go to the TruSeq DNA Sample Preparation
support page and click the Documentation & Literature tab. A MyIllumina
account is required.
Handling Liquids
Good liquid handling measures are essential, particularly when quantifying libraries or
diluting concentrated libraries for making clusters.
} Small differences in volumes (±0.5 µl) can sometimes give rise to very large
differences in cluster numbers (~100,000).
} Small volume pipetting can be a source of potential error in protocols that require
generation of standard curves, such as qPCR, or those that require small but precise
volumes, such as the Agilent Bioanalyzer.
} If small volumes are unavoidable, then due diligence should be taken to make sure
that pipettes are correctly calibrated.
} Make sure that pipettes are not used at the volume extremes of their performance
specifications.
} Care should be taken with solutions of high molecular weight double-stranded
DNA (dsDNA). These can be viscous and not evenly dispersed, resulting in aliquot
measurements that are not representative of the true concentration of the solution.
} To minimize pipetting errors, especially with small volume enzyme additions,
prepare the reagents for multiple samples simultaneously. As a result, pipette once
from the reagent tubes with a larger volume, rather than many times with small
volumes. This will allow you to aliquot in a single pipetting movement to
individual samples and standardize across multiple samples.
TruSeq DNA Sample Preparation Guide
11
Best Practices
Best Practices
Getting Started
Handling Master Mix Reagents
When handling the master mix reagents:
} Minimize freeze-thaw cycles. If you do not intend to consume the reagents in one
use, dispense the reagent into aliquots after the initial thaw and refreeze the aliquots
in order to avoid excessive freeze-thaw cycles. However, if you aliquot, you might
not have enough reagents for the full number of reactions over multiple uses.
} Add reagents in the order indicated and avoid making master-mixes containing the
in-line controls.
} Take care while adding the A-Tailing Mix (ATL) and Ligation Mix (LIG) due to the
viscosity of the reagents.
Handling Magnetic Beads
Follow appropriate handling methods when working AMPure XP Beads:
NOTE
Cleanup procedures have only been validated using the 96-well plates and
the magnetic stand specified in the Consumables and Equipment list.
Comparable performance is not guaranteed when using a microcentrifuge
tube or other formats, or other magnets.
} Prior to use, allow the beads to come to room temperature.
} Do not reuse beads. Always add fresh beads when performing these procedures.
} Immediately prior to use, vortex the beads until they are well dispersed. The color of
the liquid should appear homogeneous.
} When performing the LS protocol:
• After adding the beads to the reaction, mix the solution gently and thoroughly
by pipetting up and down 10 times, making sure the liquid comes in contact
with the beads and that the beads are resuspended homogeneously.
• Pipetting with the tips at the bottom of the well and not pipetting the entire
volume of the solution helps prevent the solution from foaming. Excessive
foaming leads to sample loss, because the foam is not transferred out of the
plate efficiently.
} When performing the HS protocol, after adding the beads to the reaction, seal the
plate and shake the plate on a microplate shaker at 1,800 rpm for 2 minutes.
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Part # 15026486 Rev. C
}
}
}
}
}
}
}
}
}
}
}
Avoiding Cross-Contamination
Practice the following to avoid cross-contamination:
} Open only one adapter tube at a time.
TruSeq DNA Sample Preparation Guide
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Best Practices
}
}
}
Repeat, if necessary, until the color of the mixture appears homogeneous after
mixing.
Take care to minimize bead loss which can impact final yields.
Change the tips for each sample.
Let the mixed samples incubate for 15 minutes at room temperature for maximum
recovery.
When aspirating the cleared solution from the reaction plate and wash step, it is
important to keep the plate on the magnetic stand and to not disturb the separated
magnetic beads. Aspirate slowly to prevent the beads from sliding down the sides
of the wells and into the pipette tips.
To prevent the carryover of beads after elution, approximately 2.5 µl of supernatant
are left when the eluates are removed from the bead pellet.
Prepare fresh 80% ethanol. Ethanol tends to absorb water from the air, therefore,
fresh 80% ethanol should be prepared for optimal results.
Be sure to remove all of the ethanol from the bottom of the wells, as it can contain
residual contaminants.
Keep the reaction plate on the magnetic stand and let it air-dry at room temperature
to prevent potential bead loss due to electrostatic forces. Allow for the complete
evaporation of residual ethanol, as the presence of ethanol will impact the
performance of the subsequent reactions. Illumina recommends at least 15 minutes
drying time, but a longer drying time might be required. Remaining ethanol can be
removed with a 20 µl pipette.
Use the Resuspension Buffer (RSB) for DNA elution.
Avoid over drying the beads, which can impact final yields.
When performing the LS protocol, resuspend the dried pellets using a single
channel or multichannel pipette.
When performing the HS protocol, resuspend the dried pellets by shaking.
When removing and discarding supernatant from the wells, use a single channel or
multichannel pipette and take care not to disturb the beads.
To maximize sample recovery during elution, incubate the sample/bead mix for 2
minutes at room temperature before placing the samples onto the magnet.
Getting Started
} Clean the bottom of the 96-well PCR plate or eight-tube strip used to pierce the foil
seal of a DNA Adapter Plate (DAP) with a sterile 70% Ethanol wipe.
} Pipette carefully to avoid spillage.
} Clean pipettes and change gloves between handling different adapter stocks.
} Clean work surfaces thoroughly before and after the procedure.
Potential DNA Contaminants
Avoid potential DNA contaminants:
} Incorrect DNA quantitation can result from DNA contamination, for example,
interference from superfluous nucleic acids in a sample (e.g., RNA, small nucleic
acid fragments, nucleotides, single-stranded DNA), excess proteins, or other
contaminating materials.
} DNA quality can also affect the quantity of usable DNA in a sample. For example, if
the DNA is damaged (e.g., heavily nicked or containing extensive
apurinic/apyrimidinic sites), many of the fragments generated may fail during
library preparation.
} High molecular weight dsDNA derived from host genomes can also interfere with
accurate quantitation. For example, bacterial artificial chromosomes (BACs) and
other bacterially-derived plasmids usually contain a small percentage of the
chromosomal DNA from the host cells, despite the best purification efforts. These
sequences might ultimately give rise to unwanted clusters on a flow cell lane.
However, this contamination can be accurately quantified by analyzing aligned
reads generated during sequencing against known bacterial sequences and
subtracting these out. High molecular weight contamination can also be estimated
prior to library preparation using qPCR assays designed to target unique
chromosomal markers.
Temperature Considerations
Temperature is an important consideration for making gDNA libraries:
} Keep libraries at temperatures ≤37°C.
} Place reagents on ice after thawing at room temperature.
} Avoid elevated temperatures, particularly in the steps preceding the adapter
ligation.
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Part # 15026486 Rev. C
Usage Guidelines
Illumina recommends these guidelines as the most efficient lab setup and pipetting
process when performing the procedures specified in Chapter 3 Low Sample (LS)
Protocol and Chapter 4 High Sample (HS) Protocol.
NOTE
The TruSeq DNA LT Sample Prep Kit contains enough of each reagent to
prepare 48 samples at one time and the TruSeq DNA HT Sample Prep Kit
contains enough reagent to prepare 96 samples at one time. If an alternate
lab setup and pipetting process is used, Illumina cannot guarantee that there
will be enough of every reagent for the full number of samples.
NOTE
When using multichannel pipettes, take care to pipette accurately into the
wells, as variations in volume will affect the sample preparation. Change tips
after each sample.
Reference the following table to determine the required reagent volume per sample for
these guidelines.
Table 6 TruSeq DNA Sample Prep Reagent Volumes
Reagent
Description
Volume per Sample (µl)
AD0XX or
DNA Adapter tube or
2.5
DAP
DNA Adapter Plate
ATL
A-Tailing Mix
12.5
CTA
A-Tailing Control
2.5
TruSeq DNA Sample Preparation Guide
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Best Practices
} When processing more than 48 samples manually, Illumina recommends
processing the plate on a bed of ice whenever possible, especially during the
enzymatic steps (when using the End Repair Mix, A-Tailing Mix, and Ligation
Mix). A large number of samples processed at room temperature may result in
uneven catalytic activity, which can lead to reduced quality of the end product.
} DNA fragments that have a high AT content are more likely to denature into single
strands than GC-rich fragments, which can result in an increased probability of
creating a bias in the sequencing coverage.
} Take care not to denature the library prior to the agarose gel electrophoresis process,
because single-stranded DNA has a different migration rate.
Getting Started
Reagent
CTE
CTL
ERP
LIG
PMM
PPC
STL
Description
End Repair Control
Ligation Control
End Repair Mix
Ligation Mix
PCR Master Mix
PCR Primer Cocktail
Stop Ligation Buffer
Volume per Sample (µl)
10
2.5
40
2.5
25
5
5
Preparing More Than 24 Samples
When preparing more than 24 samples, follow these guidelines as you perform each
procedure in the protocol. Use a multichannel pipette with eight tips to perform all
transfers from the reagent vessel to the sample plate.
Sample Distribution
Distribute each sample into a separate column of the plate. Use the appropriate plate for
the protocol being performed:
} LS protocol - 96-well 0.3 ml PCR plate
} HS protocol - 96-well MIDI plate and 96-well HSP plate
NOTE
Illumina highly recommends using the Illumina Experiment Manager and
reviewing the low-plex pooling guidelines in the Normalize and Pool Libraries
procedures when setting up the sample plate for use with a DAP. Prepare
each sample in the sample plate position that corresponds to the desired
dual-indexed DNA adapter position in the DAP.
Reagents in Reservoirs
When each of the following reagents is required in the protocol, distribute each into a
separate multichannel reagent reservoir as follows:
} 80% Ethanol
} AMPure XP Beads
} Resuspension Buffer
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Part # 15026486 Rev. C
Determine the volume needed for each of the above reagents using the equation (#
of samples x volume per sample) + 600 µl dead volume. Reference Table 6 for the
required reagent volume per sample.
2
Fill a separate multichannel reagent reservoir with the determined amount of each
reagent.
When each of the above reagents is required in the protocol, distribute each to the
sample plate as follows:
1
Using an eight tip multichannel pipette, transfer the reagent in the reservoir to the
samples in the plate as follows, while holding the pipette vertically. Reference Table
6 for the required reagent volume per sample.
Figure 1 Transfer Reagent from Reservoir to Sample Plate with 24 or More Samples
a
b
c
d
e
Pipette the required reagent volume per sample from the reservoir.
Add the reagent to column 1 of the sample plate. Change the tips.
Pipette the required reagent volume per sample from the reservoir.
Add the reagent to column 2 of the sample plate. Change the tips.
Repeat as needed for each column containing a sample.
Reagents in Strip Tubes
When the remaining reagents not mentioned above, except the adapters, are required in
the protocol, distribute each evenly across eight wells of an eight-tube strip. Add an
TruSeq DNA Sample Preparation Guide
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Best Practices
1
Getting Started
allowance of 5 µl for dead volume per well.
When each reagent in an eight-tube strip is required in the protocol, distribute each to
the sample plate as follows:
1
Using an eight tip multichannel pipette, transfer the reagent in the eight-tube strip
to the samples in the plate as follows, while holding the pipette vertically. Reference
Table 6 for the required reagent volume per sample.
Figure 2 Transfer Reagent from Strip Tube to Sample Plate with 24 or More Samples
a
b
c
d
e
Pipette the reagent from the eight strip wells.
Add the reagent to column 1 of the sample plate. Change the tips.
Pipette the reagent from the eight strip wells.
Add the reagent to column 2 of the sample plate. Change the tips.
Repeat as needed for each column containing a sample.
Index Adapters
When using DNA index adapter tubes, do one of the following:
} Add 2.5 µl of the appropriate/desired adapter index individually to each well of the
plate containing a sample, using a single channel pipette.
} Using an eight-tube strip:
• Distribute the index adapters into the wells of an eight-tube strip, with a
different adapter in each well.
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Part # 15026486 Rev. C
When using a DAP, see Handling Adapter Plate on page 42.
Preparing 12–24 Samples
When preparing 12–24 samples, follow these guidelines as you perform each procedure
in the protocol. Use a multichannel pipette with three tips to perform all transfers from
the reagent vessel to the sample plate.
Sample Distribution
Distribute the 12–24 samples into three columns and four to eight rows (e.g., four rows
per 12 samples) of the plate. Draw a line on the plate to visually separate the three
columns. Use the appropriate plate for the protocol being performed.
Figure 3 Draw Line on Plate
A
B
96-well 0.3 ml PCR plate (LS Protocol)
96-well MIDI plate and 96-well HSP plate (HS Protocol)
Reagents in Reservoirs
When each of the following reagents is required in the protocol, distribute each into a
separate multichannel reagent reservoir as follows:
} 80% Ethanol
} AMPure XP Beads
} Resuspension Buffer
TruSeq DNA Sample Preparation Guide
19
Best Practices
• Add 2.5 µl of the appropriate/desired adapter index from the well of the eighttube strip to each well of the plate containing a sample, using a multichannel
pipette.
Getting Started
1
Determine the volume needed using the equation (# of samples x volume per
sample) + 600 µl dead volume. Reference Table 6 for the required reagent volume
per sample.
2
Fill a separate multichannel reagent reservoir with the determined amount of each
reagent.
When each of the above reagents is required in the protocol, distribute each to the
sample plate as follows:
1
Using a multichannel pipette with three tips, transfer the reagent in the reservoir to
the samples in the plate as follows, while holding the pipette vertically. Reference
Table 6 for the required reagent volume per sample.
Figure 4 Transfer Reagent from Reservoir to Sample Plate with 12–24 Samples
a
b
c
d
e
Pipette the required reagent volume per sample from the reservoir.
Add the reagent to row 1 of the sample plate. Change the tips.
Pipette the required reagent volume per sample from the reservoir.
Add the reagent to row 2 of the sample plate. Change the tips.
Repeat as needed for each row containing a sample.
Reagents in Strip Tubes
When the remaining reagents not mentioned above, except the adapters, are required in
the protocol, distribute each evenly across the three wells of an eight-tube strip. Add an
allowance of 5 µl for dead volume per well.
When each reagent in an eight-tube strip is required in the protocol, distribute each to
the sample plate as follows:
1
20
Using a multichannel pipette with three tips, transfer the reagent in the eight-tube
strip to the samples in the plate as follows, while holding the pipette vertically.
Reference Table 6 for the required reagent volume per sample.
Part # 15026486 Rev. C
Best Practices
Figure 5 Transfer Reagent from Strip Tube to Sample Plate with 12–24 Samples
a
b
c
d
e
Pipette the reagent from the three strip wells.
Add the reagent to row 1 of the sample plate. Change the tips.
Pipette the reagent from the three strip wells.
Add the reagent to row 2 of the sample plate. Change the tips.
Repeat as needed for each row containing a sample.
Index Adapter Tubes
When DNA index adapter tubes are used, add 2.5 µl of the appropriate/desired adapter
index individually to each well of the plate containing a sample, using a single channel
pipette.
Preparing Less Than 12 Samples
When preparing less than 12 samples, follow these guidelines as you perform each
procedure in the protocol:
} Add each reagent individually to the samples using a single channel pipette.
} If planning more than three freeze-thaw cycles, aliquot the reagents equally into six
separate vessels.
Equipment
Review the programming instructions for your thermal cycler user guide to ensure that
it is programmed appropriately using the heated lid function.
TruSeq DNA Sample Preparation Guide
21
Getting Started
DNA Input Recommendations
It is important to quantitate the input DNA and assess the DNA quality prior to
performingTruSeq DNA Sample Preparation.
Input DNA Quantitation
Follow these DNA input recommendations:
} Correct quantification of gDNA is essential.
} 1 µg input DNA is recommended.
} The ultimate success or failure of library preparation strongly depends on using an
accurately quantified amount of input DNA.
} Illumina recommends using fluorometric based methods for quantification
including PicoGreen or Qubit to provide accurate quantification of dsDNA. UV-spec
based methods, such as the Nanodrop, will measure any nucleotides present in the
sample including RNA, dsDNA, ssDNA, and free nucleotides which can give an
inaccurate measurement of gDNA.
} Use multiple methods of quantification to validate results.
} DNA quantification methods that rely on intercalating fluorescent dyes measure
only double-stranded DNA and are less subject to excess nucleic acids.
• These methods require the preparation of calibration curves and are highly
sensitive to pipetting error.
• Make sure that pipettes are correctly calibrated and are not used at the volume
extremes of their performance specifications.
Assessing DNA Quality
} Absorbance measurements at 260 nm are commonly used to assess DNA quality:
• The ratio of absorbance at 260 nm to absorbance at 280 nm is used as an
indication of sample purity, and values of 1.8–2.0 are considered indicative of
relatively pure DNA.
• Both absorbance measurements can be compromised by the presence of RNA or
small nucleic acid fragments such as nucleotides.
• gDNA samples should be carefully collected to make sure that they are free of
contaminants.
22
Part # 15026486 Rev. C
TruSeq DNA Sample Preparation Guide
23
DNA Input Recommendations
} Gel electrophoresis is a powerful means for revealing the condition (including the
presence or absence) of DNA in a sample.
• Where possible or necessary, a gel should be run to assess the condition of the
DNA sample.
— Impurities, such as detergents or proteins, can be revealed by visible
smearing of DNA bands in the gel.
• RNA, which interferes with 260 nm readings, is often visible at the bottom of a
gel.
• A ladder or smear below a band of interest might indicate nicking or other
damage to DNA.
Getting Started
In-Line Control DNA
The End Repair Control, A-Tailing Control, and Ligation Control reagents contain DNA
fragments used as controls for the enzymatic activities of the End Repair Mix, A-Tailing
Mix, and Ligation Mix, respectively. Each reagent contains dsDNA fragments designed
to report the success or failure of a specific enzymatic activity used in the library
preparation process. Readout is determined by sequencing. If the sequence of an in-line
control appears in the final sequencing data viewed in the Sequence Analysis Viewer
(SAV), it indicates that its corresponding step was successful. If it does not, or if it
appears in substantially diminished numbers, it indicates the step failed. The controls
are intended for troubleshooting and are useful for identifying the specific mode of
failure, but are uninformative in cases where sequencing data is not generated from a
library.
NOTE
The use of these controls is optional and they can be replaced with the same
volume of Resuspension Buffer.
The control molecules work through the design of their ends. Controls are added to the
reactions just prior to their corresponding step in the protocol. Their end structures
match those of a DNA molecule that has not gone through the step. If the step is
successful, the control molecule will be modified to participate in downstream reactions
of library generation and resulting in sequencing data. If the step fails, the control
molecule will not go forward in the process and no sequencing data will be generated.
Using 1 µg of starting material, the controls yield approximately 0.2% of clusters,
although this can vary based on library yield.
Table 7 In-Line Control Functions
Reagent
Function
End Repair Mix End repair: Generate blunt
ended fragments by 3'–>5'
exonuclease and polymerase
activities
End Repair Mix End repair: Add 5'-phosphate
groups needed for
downstream ligation
24
Control
End
Repair
Control 1*
End
Repair
Control 2*
Structure of Control
DNA Ends
5' overhang at one
end, 3' overhang at
other end
Blunt with 5'-OH
group
Part # 15026486 Rev. C
A-Tailing Mix
Ligation Mix
Function
A-tailing: Make fragments
compatible with adapters and
prevent self-ligation by adding
a 3'-A overhang
Ligation: Join adapters to
inserts
Control
A-Tailing
Control
Structure of Control
DNA Ends
Blunt with 5'phosphate group
Ligation
Control
Single-base 3' 'A' base
overhang
*End Repair Control 1 and End Repair Control 2 are separate controls included in the End Repair
Control reagent
The control reagents can be used for a variety of library insert sizes. Each is provided in
ladders ranging from approximately 150–850 bp in 100 bp increments. Each control
molecule has a unique DNA sequence, indicating both its function and size. The RTA
software (version 1.9 and higher) recognizes these sequences and isolates the control
sequences from the main body of sequencing reads and reports their counts per lane in
the controls tab of the RTA status.html page. For more information regarding the control
read-out in the SAV, see the Sequence Analysis Viewer User Guide.
TruSeq DNA Sample Preparation Guide
25
In-Line Control DNA
Reagent
Getting Started
Tracking Tools
Illumina provides the following tools for sample tracking and guidance in the lab:
} Experienced User Card (EUC) to guide you through the protocol, but with less
detail than provided in this user guide. New or less experienced users are strongly
advised to follow this user guide and not the EUC.
} Lab Tracking Form (LTF) to record information about library preparation such as
operator name, sample and index information, start and stop times, reagent lot
numbers, and barcodes.
• Create a copy of the lab tracking form for each time you perform this protocol to
prepare a library for sequencing.
• Use it online and save it electronically or print it and fill it out manually.
NOTE
You can download the above TruSeq DNA Sample Preparation documents
from the Illumina website at http://www.illumina.com. Go to the TruSeq
DNA Sample Preparation support page and click the Documentation &
Literature tab. A MyIllumina account is required.
} Illumina Experiment Manager (IEM) to create your sample sheet using a wizardbased application. The sample sheet is used to record information about your
samples for later use in data analysis. The IEM guides you through the steps to
create your sample sheet based on the analysis workflow for your run. The IEM
provides a feature for recording parameters for your sample plate, such as sample
ID, dual indices, and other parameters applicable to your 96-well plate.
• When prompted to select an Assay in IEM, choose:
— TruSeq LT if you are using the TruSeq DNA LT Sample Prep Kit
— TruSeq HT if you are using the TruSeq DNA HT Sample Prep Kit
NOTE
IEM can be run on any Windows platform. You can download it from the
Illumina website at http://www.illumina.com. A MyIllumina account is
required.
26
Part # 15026486 Rev. C
Check to make sure that you have all of the reagents identified in this section before
proceeding. The 48 samples kits are available as Set A and B, which differ in the indices
provided and together allow for pooling of up to 24 samples.
Table 8 TruSeq DNA Sample Preparation Kits
Kit Name
Catalog #
Number
of
Samples
Supported
Number
of
Indices
TruSeq DNA LT Sample
Prep Kit - Set A
FC-121-2001
48
12
TruSeq DNA LT Sample
Prep Kit - Set B
FC-121-2002
48
12
TruSeq DNA HT Sample
Prep Kit
FC-121-2003
96
96
TruSeq DNA LT Sample Prep Kit
The TruSeq DNA LT Sample Prep Kit contains two boxes: a Set A or Set B box and a
PCR box.
48 Samples - Set A Box or Set B Box
You will receive either box A or B with the kit depending on the set ordered. These
boxes also contain plate barcode labels.
Store at -15° to -25°C
These boxes are shipped on dry ice. As soon as you receive them, store the following
components at -15° to -25°C.
TruSeq DNA Sample Preparation Guide
27
Kit Contents
Kit Contents
Getting Started
Set A
Figure 6 TruSeq DNA LT Sample Prep Kit, 48 Samples-Set A Box, part # 15025064
Slot
1
2
3
4
5
6
7
8
9
10
11
12
13
14
15
16
17
18
19
20
28
Reagent
RSB
ERP
ATL
LIG
CTE
CTA
CTL
STL
AR002
AR004
AR005
AR006
AR007
AR012
AR013
AR014
AR015
AR016
AR018
AR019
Part #
15026770
15012494
15012495
15026773
15026774
15026775
15026776
15012546
15026621
15026623
15026624
15026625
15026627
15026632
15024641
15024642
15024643
15024644
15024646
11324647
Description
Resuspension Buffer
End Repair Mix
A-Tailing Mix
Ligation Mix
End Repair Control
A-Tailing Control
Ligation Control
Stop Ligation Buffer
DNA Adapter Index 2
DNA Adapter Index 4
DNA Adapter Index 5
DNA Adapter Index 6
DNA Adapter Index 7
DNA Adapter Index 12
DNA Adapter Index 13
DNA Adapter Index 14
DNA Adapter Index 15
DNA Adapter Index 16
DNA Adapter Index 18
DNA Adapter Index 19
Part # 15026486 Rev. C
Kit Contents
Set B
Figure 7 TruSeq DNA LT Sample Prep Kit, 48 Samples-Set B Box, part # 15025065
Slot
1
2
3
4
5
6
7
8
9
10
11
12
13
14
15
16
17
18
19
20
Reagent
RSB
ERP
ATL
LIG
CTE
CTA
CTL
STL
AD001
AD003
AD008
AD009
AD010
AD011
AD020
AD021
AD022
AD023
AD025
AD027
TruSeq DNA Sample Preparation Guide
Part #
15026770
15012494
15012495
15026773
15026774
15026775
15026776
15012546
15026620
15026622
15026628
15026629
15026630
15026631
15024648
15024649
15024650
15024651
15024653
11324654
Description
Resuspension Buffer
End Repair Mix
A-Tailing Mix
Ligation Mix
End Repair Control
A-Tailing Control
Ligation Control
Stop Ligation Buffer
DNA Adapter Index 1
DNA Adapter Index 3
DNA Adapter Index 8
DNA Adapter Index 9
DNA Adapter Index 10
DNA Adapter Index 11
DNA Adapter Index 20
DNA Adapter Index 21
DNA Adapter Index 22
DNA Adapter Index 23
DNA Adapter Index 25
DNA Adapter Index 27
29
Getting Started
48 Samples - PCR Box Store at -15° to -25°C
This box is shipped on dry ice. As soon as you receive it, store the following
components at -15° to -25°C.
Figure 8 TruSeq DNA LT Sample Prep Kit, 48 Samples-PCR Box, part # 15027084
Slot
1
2
Reagent
PMM
PPC
Part #
15026785
15031748
Description
PCR Master Mix
PCR Primer Cocktail
TruSeq DNA HT Sample Prep Kit
The TruSeq DNA HT Sample Prep Kit contains two boxes: a Core-PCR box and an
Adapter Plate box.
96 Samples - Core-PCR Box
Store at -15° to -25°C
This box is shipped on dry ice. As soon as you receive it, store the following
components at -15° to -25°C. This box also contains plate barcode labels.
30
Part # 15026486 Rev. C
Slot
1–2
3–4
5–6
7–8
9–10
11–12
13–14
15–16
17–18
19–20
Reagent
RSB
ERP
ATL
LIG
CTE
CTA
CTL
STL
PMM
PPC
Part #
15026770
15012494
15012495
15026773
15026774
15026775
15026776
15012546
15026785
15031748
Description
Resuspension Buffer
End Repair Mix
A-Tailing Mix
Ligation Mix
End Repair Control
A-Tailing Control
Ligation Control
Stop Ligation Buffer
PCR Master Mix
PCR Primer Cocktail
96 Samples- Adapter Plate Box
Store at -15° to -25°C
This box is shipped on dry ice. As soon as you receive it, store the contents at -15° to
Ȭ25°C.
Figure 10 TruSeq DNA HT Sample Prep Kit, 96 Samples - Adapter Plate Box, part # 15032317
Slot
1
Reagent
DAP
TruSeq DNA Sample Preparation Guide
Part #
Description
15016426 DNA Adapter Plate, 96plex
31
Kit Contents
Figure 9 TruSeq DNA HT Sample Prep Kit, 96 Samples - Core-PCR Box, part # 15032316
Getting Started
Consumables and Equipment
Check to make sure that you have all of the necessary user-supplied consumables and
equipment before proceeding to the TruSeq DNA Sample Preparation protocol. The
requirement of some supplies are dependent upon the protocol performed (LS or HS)
and these items are specified in separate tables below.
Table 9 User-Supplied Consumables
32
Consumable
Supplier
10 µl barrier pipette tips
General lab supplier
10 µl multichannel pipettes
General lab supplier
10 µl single channel pipettes
General lab supplier
1000 µl barrier pipette tips
General lab supplier
1000 µl multichannel pipettes
General lab supplier
1000 µl single channel pipettes
General lab supplier
20 µl barrier pipette tips
General lab supplier
20 µl multichannel pipettes
General lab supplier
20 µl single channel pipettes
General lab supplier
200 µl barrier pipette tips
General lab supplier
200 µl multichannel pipettes
General lab supplier
200 µl single channel pipettes
General lab supplier
6X gel loading dye
BioLabs, catalog #
B7021S
50 X TAE buffer
Bio-Rad, part # 161-0743
Part # 15026486 Rev. C
Supplier
96-well storage plates, round well,
0.8 ml (“MIDI” plate)
Fisher Scientific,
part # AB-0859
Agencourt AMPure XP 60 ml kit
Beckman Coulter
Genomics,
part # A63881
BenchTop 100 bp DNA ladder
Promega, part # G829B
Certified low-range ultra agarose
Bio-Rad, part # 161-3107
Clean scalpels
General lab supplier
MicroTube (6x16mm), AFA fiber
with crimp-cap
Covaris, part # 520052
Distilled water
General lab supplier
Ethanol 200 proof (absolute)
for molecular biology (500 ml)
Sigma Aldrich,
part # E7023
Microseal ‘B’ adhesive seals
BioRad,
part # MSB-1001
MinElute Gel Extraction Kit
QIAGEN, part# 28604
Paired-End Sample Prep Kit
(Optional -for alternative fragmentation by
nebulization only)
Illumina,
10 samples
catalog # PE-102-1001
40 samples,
catalog # PE-102-1002
PCR grade water (for gel-free method)
General lab supplier
QIAquick PCR Purification Kit
(Optional - for alternative fragmentation by
nebulization only)
QIAGEN, part # 28104
TruSeq DNA Sample Preparation Guide
Consumables and Equipment
Consumable
33
Getting Started
Consumable
Supplier
Qubit dsDNA BR Assay Kit
Life Technologies
100 assays,
catalog # Q32850
500 assays,
catalog # Q32853
Qubit assay tubes or
Axygen PCR-05-C tubes
Life Technologies,
catalog # Q32856 or
VWR, part # 10011-830
RNase/DNase-free multichannel reagent reservoirs,
disposable
VWR, part # 89094-658
RNase/DNase-free 8-well PCR strip tubes and caps
General lab supplier
RNase/DNase zapper
(to decontaminate surfaces)
General lab supplier
SyBr Gold Nucleic acid gel stain
Invitrogen,
part # S11494
Tris-Cl 10 mM, pH8.5
with 0.1% Tween 20
General lab supplier
Tween 20
Sigma, part # P7949
Ultra pure water
General lab supplier
Table 10 User-Supplied Consumables - Additional Items for LS Processing
34
Consumable
Supplier
96-well 0.3 ml skirtless PCR plates, or
Twin.Tec 96-well PCR plates
E&K Scientific, part # 480096
Eppendorf, part # 951020303
Part # 15026486 Rev. C
Consumables and Equipment
Table 11 User-Supplied Consumables - Additional Items for HS Processing
Consumable
Supplier
Microseal 96-well PCR plates
(“HSP” plate)
Bio-Rad, part # HSP-9601
Microseal ‘A’ film
Bio-Rad, part # MSA-5001
Table 12 User-Supplied Equipment
Equipment
Supplier
96-well thermal cycler
(with heated lid)
General lab supplier
Covaris S220 or
Covaris E220
Covaris, part # SE-501-1001 or
Covaris, part # SE-501-1002
Dark reader
transilluminator
Clare Chemical Research, part # DR195M
Electrophoresis power
supply
General lab supplier
Magnetic stand-96
Life Technologies, catalog # AM10027
Microplate centrifuge
General lab supplier
Qubit 2.0 Fluorometer
Life Technologies, catalog # Q32866
http://products.invitrogen.com/ivgn/product/Q32866
Thermo Scientific Owl B2
EasyCast Mini Gel System
(US) Thermo Scientific, part # B2, or
Fisher Scientific, part # 09-528-110B
(Other Regions) Fisher Scientific,
part # OWL-130-101J B
Vortexer
General lab supplier
TruSeq DNA Sample Preparation Guide
35
Getting Started
Table 13 User-Supplied Equipment - Additional Items for HS Processing
36
Consumable
Supplier
High Speed Micro Plate Shaker
VWR, catalog # 13500-890 (110V/120V)
VWR, catalog # 14216-214 (230V)
MIDI plate insert for heating system
Illumina, catalog # BD-60-601
Stroboscope
General lab supplier
Tru Temp Microheating System
Illumina, catalog # SC-60-503 (115V)
Illumina, catalog # SC-60-504 (220V)
Part # 15026486 Rev. C
Indexed Adapter Sequences
Indexed Adapter Sequences
This section details the indexed adapter sequences.
TruSeq DNA LT Sample Prep Kit Indexed Adapter Sequences
The TruSeq DNA LT Sample Prep Kit contains the following the indexed adapter
sequences. The set (A or B) containing the adapter is also specified.
NOTE
• The index numbering is not contiguous. Index 17, 24, and 26 are skipped.
• The base in parentheses () indicates the base for the seventh cycle and is
not considered as part of the index sequence. The index should be
recorded in the sample sheet as only six bases. For indexes 13 and above,
the seventh base (in parentheses) might not be A, and this will be seen in
the seventh cycle of the index read.
Table 14 TruSeq DNA LT Sample Prep Kit Indexed Adapter Sequences
Adapter
Sequence
Set
Adapter
Sequence
Set
AD001
ATCACG(A)
B
AD013
AGTCAA(C)
A
AD002
CGATGT(A)
A
AD014
AGTTCC(G)
A
AD003
TTAGGC(A)
B
AD015
ATGTCA(G)
A
AD004
TGACCA(A)
A
AD016
CCGTCC(C)
A
AD005
ACAGTG(A)
A
AD018
GTCCGC(A)
A
AD006
GCCAAT(A)
A
AD019
GTGAAA(C)
A
AD007
CAGATC(A)
A
AD020
GTGGCC(T)
B
AD008
ACTTGA(A)
B
AD021
GTTTCG(G)
B
TruSeq DNA Sample Preparation Guide
37
Getting Started
Adapter
Sequence
Set
Adapter
Sequence
Set
AD009
GATCAG(A)
B
AD022
CGTACG(T)
B
AD010
TAGCTT(A)
B
AD023
GAGTGG(A)
B
AD011
GGCTAC(A)
B
AD025
ACTGAT(A)
B
AD012
CTTGTA(A)
A
AD027
ATTCCT(T)
B
TruSeq DNA HT Sample Prep Kit Indexed Adapter Sequences
The DAP in the TruSeq DNA HT Sample Prep Kit contains the following the indexed
adapter sequences:
NOTE
The Index recorded in the sample sheet is the full 8 bases and 8 bases are
sequenced per indexed read.
Table 15 TruSeq DNA HT Sample Prep Kit Indexed Adapter Sequences
38
Indexed Adapter 1
Sequence
Indexed Adapter 2
Sequence
D701
ATTACTCG
D501
TATAGCCT
D702
TCCGGAGA
D502
ATAGAGGC
D703
CGCTCATT
D503
CCTATCCT
D704
GAGATTCC
D504
GGCTCTGA
D705
ATTCAGAA
D505
AGGCGAAG
D706
GAATTCGT
D506
TAATCTTA
D707
CTGAAGCT
D507
CAGGACGT
D708
TAATGCGC
D508
GTACTGAC
Part # 15026486 Rev. C
Sequence
D709
CGGCTATG
D710
TCCGCGAA
D711
TCTCGCGC
D712
AGCGATAG
TruSeq DNA Sample Preparation Guide
Indexed Adapter 2
Indexed Adapter Sequences
Indexed Adapter 1
Sequence
39
Getting Started
Adapter Options
Illumina provides two methods for indexing samples to perform pooled sequencing,
using either DNA Adapter Index tubes or a DAP.
Adapter Tubes
The TruSeq DNA LT Sample Prep Kit contains DNA Adapter Index tubes that can be
used to perform pooled sequencing.
} Each tube contains a unique single 6 base index adapter on the P7 strand and
contains enough reagent for eight reactions.
} Samples prepared with these adapters can be sequenced on any Illumina
sequencing platform using the 7 cycle Single Index Recipe.
For more information on pooling guidelines when using adapter index tubes, see
Adapter Tube Pooling Guidelines on page 45.
For more information on sequencing samples prepared using the TruSeq DNA LT
Sample Prep Kit, see your sequencing platform user guide.
Adapter Plate
The TruSeq DNA HT Sample Prep Kit contains a DAP, which is a 96-well plate
containing 96 uniquely indexed adapter combinations designed for manual or
automated preparation of 96 uniquely indexed samples.
} Each well of the plate is single-use and the plate can undergo up to 4 freeze/thaw
cycles.
} The DNA adapters provided in this plate are dual-indexed, meaning that each
adapter contains two indices. These are referred to as Index 1(i7), an 8 base Index
on the P7 strand, and Index 2(i5), an 8 base Index on the P5 strand.
} There are 12 Index 1 sequences (D701-D712) arrayed across the columns and 8
Index 2 sequences (D501-D508) arrayed down the rows, to generate 96 uniquely
dual-indexed adapter combinations in the plate.
} If compatible, samples prepared with these adapters can be sequenced on an
Illumina sequencing platform using the dual-indexed recipes for dual indexing or
the 8 cycle single-indexed recipe for single indexing.
40
Part # 15026486 Rev. C
For more information on sequencing samples prepared using the TruSeq DNA HT
Sample Prep Kit, see your sequencing platform user guide.
Table 16 Dual-Indexed Sequencing Platform Compatibility
Platform
Compatibility
MiSeq®
Full compatibility
HiSeq®
• Requires TruSeq Dual Index Sequencing Primer Box, Single Read for
dual-indexed sequencing on a single-read flow cell.a
• Requires HCS 1.5/RTA 1.13 or later
• Process with OLB 1.9.3 or later if offline base call is needed
• Process with CASAVA 1.8.2 or later
Genome
Analyzer
• Requires TruSeq Dual Index Sequencing Primer Box, Single Read for
dual-indexed sequencing on a single-read flow cell.a
• Requires SCS 2.10/RTA 1.13 or later
• Process with OLB 1.9.4 or later if offline base call is needed
• Process with CASAVA 1.8.2 or later
™
a. Not required for sequencing on paired-end flow cells.
Pooling Preparation with Adapter Plate
The TruSeq DNA HT Sample Prep Kit contains a DAP and enables preparation of up to
96 libraries with unique dual indexes.
TruSeq DNA Sample Preparation Guide
41
Adapter Options
For more information on pooling guidelines when using the DAP, see Adapter Plate
Pooling Guidelines on page 46.
Getting Started
Figure 11
DAP Dual-Indexed Layout
When less than the full set of 96 libraries are pooled and sequenced, it is extremely
important that libraries with compatible index combinations are used in the indexed
pool. Illumina strongly recommends the following planning steps before beginning
library preparation:
1
Determine the number of libraries that will be pooled for sequencing.
2
Ensure that the pool contains the required index combinations, as described in
Adapter Plate Pooling Guidelines on page 46. Select the DNA index adapters based on
the same guidelines.
3
Use the Illumina Experiment Manager to create a sample sheet which will be used
during the sequencing run. This step also identifies any incorrect index
combinations, allowing re-design before library preparation starts. For more
information, see Tracking Tools on page 26.
4
Use the Lab Tracking Form or sample plate generator from the Illumina Experiment
Manager to specify the layout of all sample plates in 96-well plate format for
compatibility with the 96-well DAP. Arrange samples that will be pooled together in
the same orientation as the indices in the DAP. For more information, see Tracking
Tools on page 26.
Handling Adapter Plate
The DAP is designed for use in the TruSeq DNA Sample Prep high sample protocol.
} The DAP is single-use for each well.
42
Part # 15026486 Rev. C
Prepare Adapter Plate
Prepare the DAP for use as follows:
1
Thaw the plate for 10 minutes at room temperature on the benchtop. Visually
inspect the wells to ensure that they all are completely thawed.
2
Remove the adapter plate tape seal.
3
Centrifuge the plate at 280 xg for 1 minute to collect all of the adapter to the bottom
of the well.
4
Remove the plastic cover and save the cover if you are not processing the entire
plate at once.
5
Apply the DAP barcode label to the DAP.
If using only part of the DAP, it may be useful to use a lab pen to mark on the foil
seal the adapter wells being used. When doing so, be careful not to pierce the foil
seal.
Pierce Adapter Plate Seal
Pierce the DAP foil seal as follows:
1
Place the DAP on the benchtop so that the part number barcode on the long side of
the plate is facing you and the clipped corner is located on the lower left.
Figure 12 Correct DAP Orientation
2
Do one of the following:
TruSeq DNA Sample Preparation Guide
43
Adapter Options
} Illumina recommends that the DAP does not undergo more than 4 freeze/thaw
cycles.
} To maximize the use of the DAP, process more than 24 samples at a time. These
samples can then be pooled in any supported configuration.
Getting Started
— If using the entire plate at once, use the bottom of a clean 96-well semiskirted PCR plate to pierce a hole in all of the well seals simultaneously by
gently but firmly pressing the clean plate over the foil seal.
— If using only part of the plate, use the bottom of a clean eight-tube strip,
with caps attached, to pierce holes in the desired columns that will be used
for ligation. Repeat with a new, clean eight-tube strip, with caps attached,
for each column of adapters that will be used for ligation.
} Once the foil seal has been pierced for a well, Illumina does not recommend reusing
the dual-indexed adapter from that well in future sample preparations.
Pipette Adapter Plate
Pipette the adapters from the DAP into the ligation reaction as follows, while keeping
the plate in the same orientation:
1
Using an 8-tip multichannel pipette, transfer the thawed adapter from the DAP well
to each well of the sample plate.
2
Change pipette tips between wells of the DAP. This is critical to avoid crosscontamination between wells.
3
Aspirate each dual-indexed adapter by column.
4
Discard the tips after pipetting into the ligation reaction.
Adapter Plate Storage
If not all adapter wells are used in a single experiment (< 96 samples), the plate can be
stored for future use of unused wells as follows:
1
Wipe the foil seal covering unused wells with a sterile 70% Ethanol wipe.
2
Allow the foil seal to dry.
3
Put the plastic cover that came with the DAP back on the plate.
4
Store at -15° to -25°C.
NOTE
Do not reseal the plate with a disposable seal. This will rip the original foil
seal when the disposable seal is removed for future uses.
44
Part # 15026486 Rev. C
Illumina uses a green laser to sequence G/T and a red laser to sequence A/C. At each
cycle at least one of two nucleotides for each color channel needs to be read to ensure
proper image registration. It is important to maintain color balance for each base of the
index read being sequenced, otherwise index read sequencing could fail due to
registration failure. Follow these low plex pooling guidelines, depending on the TruSeq
DNA Sample Prep kit you are using.
Adapter Tube Pooling Guidelines
When using the index adapter tubes from the TruSeq DNA LT Sample Prep Kit, follow
these pooling guidelines for single-indexed sequencing. The TruSeq DNA LT Sample
Prep Kit Set A and B, each contain 12 unique index adapter tubes. When designing lowplexity index pools for single-indexed sequencing, always use at least two unique and
compatible barcodes for each index sequenced. The following table describes possible
pooling strategies for 2–4 samples generated with the adapter index tubes in each set.
} For 5–11plex pools, use 4-plex options with any other available adapters
} Not all color-balanced pools are listed. Check the color balance of such userdesigned pools using the Illumina Experiment Manager's sample sheet generator.
Table 17 Single-Indexed Pooling Strategies for 2–4 Samples
Plexity Option
Set A Only
Set B Only
2
1
AD006 and AD012
Not recommended
2
AD005 and AD019
3
1
AD002 and AD007 and AD019
AD001 and AD010 and AD020
2
AD005 and AD006 and AD015
AD003 and AD009 and AD025
3
2-plex options with any other
AD008 and AD011 and AD022
adapter
4
1
AD005 and AD006 and AD012
AD001 and AD008 and AD010
and AD019
and AD011
2
AD002 and AD004 and AD007
AD003 and AD009 and AD022
and AD016
and AD027
3
3-plex options with any other
3-plex options with any other
adapter
adapter
TruSeq DNA Sample Preparation Guide
45
Pooling Guidelines
Pooling Guidelines
Getting Started
For more information on the Single-Indexed Sequencing workflow, see the Illumina
HiSeq, HiScan®, and Genome Analyzer user guides.
Adapter Plate Pooling Guidelines
When using the the DAP from the TruSeq DNA HT Sample Prep Kit, follow these
pooling guidelines. In addition, please review Handling Adapter Plate on page 42 and
Pooling Preparation with Adapter Plate on page 41.
Single-Indexed Sequencing
Follow the single-indexed sequencing workflow when pooling 12 or fewer samples.
When designing low plexity index pools, always use at least two unique and
compatible barcodes for each index sequenced. The following figures illustrate possible
pooling strategies for 2–12 samples generated with the DAP.
} Color balanced pools are shaded light gray with green wells.
} For 5-plex pools, dark gray wells are not used for pooled sequencing. They are
available for individual sequencing.
} For 7–11plex pools, combine any of the 2–6plex pools.
} Not all color-balanced pools are illustrated. Check the color balance of such userdesigned pools using the Illumina Experiment Manager's sample sheet generator.
For more information on the single-indexed sequencing workflow, see the Illumina
HiSeq, HiScan, and Genome Analyzer user guides.
46
Part # 15026486 Rev. C
Pooling Guidelines
Figure 13 Single-Indexed–2-plex
Figure 14 Single-Indexed–3-plex
TruSeq DNA Sample Preparation Guide
47
Getting Started
Figure 15 Single-Indexed–4-plex
Figure 16 Single-Indexed–5-plex
48
Part # 15026486 Rev. C
Pooling Guidelines
Figure 17 Single-Indexed–6-plex
Figure 18 Single-Indexed–12-plex
Dual-Indexed Sequencing
Follow the dual-indexed sequencing workflow when pooling more than 12 samples.
When designing the low-plexity index pools, always use at least two unique and
compatible barcodes for each index sequenced. The following figures illustrate possible
pooling strategies for 2–16 samples generated with the DAP.
TruSeq DNA Sample Preparation Guide
49
Getting Started
} Color balanced pools are shaded light gray with green wells. The 2-plex pools are
diagonal and shaded in light or dark gray with green wells.
} Odd numbered pools display dark gray wells that are not used for pooled
sequencing. They are available for individual sequencing.
} Not all color-balanced pools are illustrated. Check the color balance of such userdesigned pools using the Illumina Experiment Manager's sample sheet generator.
For more information on the dual-indexed sequencing workflow, see the Illumina HiSeq,
HiScan, Genome Analyzer, and MiSeq user guides.
Figure 19 Dual-Indexed–2-plex
Figure 20 Dual-Indexed–3-plex
50
Part # 15026486 Rev. C
Pooling Guidelines
Figure 21 Dual-Indexed–4-plex
Figure 22 Dual-Indexed–5-plex
TruSeq DNA Sample Preparation Guide
51
Getting Started
Figure 23 Dual-Indexed–6-plex
Figure 24 Dual-Indexed–7-plex
52
Part # 15026486 Rev. C
Pooling Guidelines
Figure 25 Dual-Indexed–8-plex, Option 1
Figure 26 Dual-Indexed–8-plex, Option 2
TruSeq DNA Sample Preparation Guide
53
Getting Started
Figure 27 Dual-Indexed–12-plex
Figure 28 Dual-Indexed–16-plex
54
Part # 15026486 Rev. C
Chapter 3 Low Sample (LS) Protocol
Introduction
Sample Prep Workflow
Fragment DNA
Perform End Repair
Adenylate 3' Ends
Ligate Adapters
Purify Ligation Products (gel method only)
Enrich DNA Fragments
Validate Library
Normalize and Pool Libraries
TruSeq DNA Sample Preparation Guide
56
58
59
63
67
69
76
80
84
87
55
Chapter 3
Low Sample (LS) Protocol
Low Sample (LS) Protocol
Introduction
This chapter describes the TruSeq DNA Sample Preparation low sample (LS) protocol.
Illumina recommends the following kit, sample number, and protocol combinations:
Table 18 Kit and Sample Number Recommendations
Number of Samples
Processed
At One Time
Kit
Recommended
<24
LT
24–48
LT or HT
>48
HT
Table 19 Kit and Protocol Recommendations
Kit
Number of
Samples
Supported
Number of Samples
Processed
At One Time
Protocol
LT
48
≤48
LS
>48
HS
≤48
LS
>48
HS
HT
96
} Review Best Practices on page 11 before proceeding.
} Follow the protocols in the order shown, using the specified volumes and
incubation parameters.
} For optimal sample tracking and quality control, fill out the Lab Tracking Form as
you perform the sample preparation. For more information, see Tracking Tools on
page 26.
} If you are pooling using adapter index tubes, record information about your
samples before beginning library preparation for later use in data analysis. For more
56
Part # 15026486 Rev. C
TruSeq DNA Sample Preparation Guide
57
Introduction
information, see Tracking Tools on page 26. Illumina recommends arranging
samples that will be combined into a common pool in the same row. Each column
should contain a common index. This will facilitate pipetting operations when
dispensing indexed adapters and pooling indexed libraries later in the protocol.
} If you are pooling with the DAP, please review the planning steps in Pooling
Preparation with Adapter Plate on page 41 before beginning library preparation.
Low Sample (LS) Protocol
Sample Prep Workflow
The following figure illustrates the processes of the TruSeq DNA Sample Preparation LS
protocol to prepare templates using 24 indexed adapter tubes or a DAP.
Figure 29 TruSeq DNA Sample Preparation LS Workflow
58
Part # 15026486 Rev. C
This process describes how to optimally fragment the gDNA depending on the
downstream application. Covaris shearing generates dsDNA fragments with 3' or 5'
overhangs. The fragmentation process described below was optimized to obtain final
libraries with the following differences:
Table 20 Fragmentation Method Options
Whole-genome
Resequencing
Gel Method
Covaris Shearing
Duration
Insert Size
40 seconds
300–400 bp
TruSeq Enrichment
Gel-free
Gel Method
Method
120 seconds
100–900 bp
200–300 bp
NOTE
If fragmenting using a nebulization technique, skip this procedure and
perform the Appendix A Alternate Fragmentation Protocols. The
nebulization procedures have only been validated for whole-genome
resequencing or enrichment with the gel-method.
Calculate the amount of DNA to be fragmented based on 1 µg input DNA for each
sample.
Illumina-Supplied Consumables
}
}
}
}
Resuspension Buffer (RSB) (1 tube)
CFP (Covaris Fragmentation Plate) barcode label
DNA (DNA Plate) barcode label
IMP (Insert Modification Plate) barcode label
User-Supplied Consumables
} 96-well 0.3 ml PCR plates (2)
} Covaris Tubes
} DNA samples
TruSeq DNA Sample Preparation Guide
59
Fragment DNA
Fragment DNA
Low Sample (LS) Protocol
Preparation
} Review DNA Input Recommendations on page 22.
} Remove one tube of Resuspension Buffer from -15° to -25°C storage and thaw it at
room temperature.
NOTE
The Resuspension Buffer can be stored at 2° to 8°C after the initial thaw.
} Turn on the Covaris instrument at least 30 minutes before starting.
• Following the manufacturer’s instructions, de-gas and pre-chill the water to a
temperature of 3° to 6°C. You can start the fragmentation procedure at 6°C.
} Apply a CFP barcode label to the Covaris tube plate.
} Apply a DNA barcode label to a new 96-well 0.3 ml PCR plate.
} Apply a IMP barcode label to a new 96-well 0.3 ml PCR plate.
Make CFP
1
Illumina recommends to quantify gDNA samples using a fluorometric-based
method such as Qubit or PicoGreen.
2
Illumina recommends to normalize the gDNA samples to a final volume of 55 µl at
20 ng/µl into each well of the new 0.3 ml PCR plate labeled with the DNA barcode.
Fragment DNA
1
Shear 1 µg of gDNA sample by transferring 52.5 µl of each DNA sample from the
DNA plate to each Covaris tube in the new 0.3 ml PCR plate labeled with CFP
barcode.
NOTE
Load the DNA sample into the Covaris tube very slowly to avoid creating
air bubbles. However, air bubbles might not be preventable during the
process run.
2
60
Fragment the DNA using the following settings:
Part # 15026486 Rev. C
Fragment DNA
Table 21 Covaris S220 or Covaris E220 Settings
Whole-genome
Resequencing
TruSeq
Enrichment
Duty factor
10%
10%
Peak Incident
Power
175
175
Cycles per burst
200
200
40 seconds
2 x 60 seconds
(120 seconds total)
Setting
Duration
Mode
Temperature
Frequency sweeping
Frequency
sweeping
5.5° to 6°C
5.5° to 6°C
Table 22 Covaris S2 or E210 Settings
Whole-genome
Resequencing
TruSeq
Enrichment
Duty cycle
10%
10%
Intensity
5.0
5.0
Cycles per
burst
200
200
40 seconds
2 x 60 seconds
(120 seconds total)
Setting
Duration
Mode
Displayed
Power
Temperature
TruSeq DNA Sample Preparation Guide
Frequency sweeping
Frequency
sweeping
Covaris S2 - 23W
Covaris E210 - 18W
Covaris S2 - 23W
Covaris E210 18W
5.5° to 6°C
5.5° to 6°C
61
Low Sample (LS) Protocol
3
Seal the Covaris tubes and centrifuge to 600 xg for 1 minute.
4
Transfer 50 µl of fragmented DNA from each Covaris tube in the CFP plate to the
corresponding well of the new 0.3 ml PCR plate labeled with the IMP barcode using
a single channel pipette.
NOTE
• When indexing libraries using adapter index tubes, Illumina recommends
arranging samples that will be combined into a common pool in the
same row. Each column should contain a common index. This will
facilitate pipetting operations when dispensing indexed adapters and
pooling indexed libraries later in the protocol.
• When indexing libraries with the DAP, arrange samples that will be
pooled together in the same orientation as the indices in the DAP.
62
Part # 15026486 Rev. C
This process converts the overhangs resulting from fragmentation into blunt ends using
an End Repair Mix. The 3' to 5' exonuclease activity of this mix removes the 3'
overhangs and the polymerase activity fills in the 5' overhangs.
Illumina-Supplied Consumables
}
}
}
}
(Optional) End Repair Control (CTE) (1 tube per 48 reactions)
End Repair Mix (ERP) (1 tube per 48 reactions)
Resuspension Buffer (RSB) (1 tube)
ALP (Adapter Ligation Plate) barcode label
User-Supplied Consumables
}
}
}
}
}
}
}
96-well 0.3 ml PCR plate
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘B’ Adhesive Seal
PCR Grade Water (for gel-free method for enrichment only)
RNase/DNase-free Reagent Reservoirs (if using multichannel pipettes)
RNase/DNase-free Strip Tubes and Caps (if using multichannel pipettes)
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
• End Repair Control
• End Repair Mix
NOTE
The use of the End Repair Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Review Handling Magnetic Beads on page 12.
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Pre-heat the thermal cycler to 30°C.
} Choose the thermal cycler pre-heat lid option and set to 100°C
TruSeq DNA Sample Preparation Guide
63
Perform End Repair
Perform End Repair
Low Sample (LS) Protocol
} Apply a ALP barcode label to a new 96-well 0.3 ml PCR plate.
Make IMP
1
Do one of the following:
• If using the in-line control reagent:
— Centrifuge the thawed End Repair Control tube to 600 xg for 5 seconds.
— Add 10 µl of thawed End Repair Control to each well of the IMP plate that
contains 50 µl of fragmented DNA.
• If not using the in-line control reagent, add 10 µl of Resuspension Buffer to each
well of the IMP plate that contains 50 µl of fragmented DNA.
2
Add 40 µl of End Repair Mix to each well of the IMP plate containing the
fragmented DNA. Gently pipette the entire volume up and down 10 times to mix
thoroughly.
3
Seal the IMP plate with a Microseal ‘B’ adhesive seal.
Incubate 1 IMP
1
Place the sealed IMP plate on the pre-heated thermal cycler. Close the lid and
incubate at 30°C for 30 minutes.
2
Remove the IMP plate from the thermal cycler.
Clean Up IMP
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
64
1
Remove the adhesive seal from the IMP plate.
2
Vortex the AMPure XP Beads until they are well dispersed.
3
Do one of the following:
• If using the gel-free method:
— Determine the amount of AMPure XP beads and PCR grade water needed
to combine to prepare a diluted bead mixture:
AMPure XP beads: # of samples X 160 µl x 0.85 = µl AMPure XP beads. For
Part # 15026486 Rev. C
4
Incubate the IMP plate at room temperature for 15 minutes.
5
Place the IMP plate on the magnetic stand at room temperature for 15 minutes or
until the liquid appears clear.
6
Using a 200 µl single channel or multichannel pipette set to 127.5 µl, remove and
discard 127.5 µl of the supernatant from each well of the IMP plate.
7
Repeat step 6 once.
NOTE
Leave the IMP plate on the magnetic stand while performing the following
80% EtOH wash steps (8–10).
8
With the IMP plate on the magnetic stand, add 200 µl of freshly prepared 80%
EtOH to each well with a sample without disturbing the beads.
9
Incubate the IMP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well. Take care not to disturb the beads.
10 Repeat steps 8 and 9 once for a total of two 80% EtOH washes.
11 Let the IMP plate stand at room temperature for 15 minutes to dry, then remove the
plate from the magnetic stand.
12 Resuspend the dried pellet in each well with 17.5 µl Resuspension Buffer. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
13 Incubate the IMP plate at room temperature for 2 minutes.
14 Place the IMP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
TruSeq DNA Sample Preparation Guide
65
Perform End Repair
example, 1.632 ml of AMPure XP beads are needed for 12 samples.
PCR grade water: # of samples X 160 µl x 0.15 = µl PCR grade water. For
example, 288 µl of PCR grade water is needed for 12 samples.
— Add 160 µl of the diluted bead mixture to each well of the IMP plate
containing 100 µl of End Repair Mix. Gently pipette the entire volume up
and down 10 times to mix thoroughly.
• If using the gel method, add 160 µl well-mixed AMPure XP Beads to each well
of the IMP plate containing 100 µl of End Repair Mix. Gently pipette the entire
volume up and down 10 times to mix thoroughly.
Low Sample (LS) Protocol
15 Transfer 15 µl of the clear supernatant from each well of the IMP plate to the
corresponding well of the new 0.3 ml PCR plate labeled with the ALP barcode.
SAFE STOPPING POINT
If you do not plan to proceed to Adenylate 3' Ends on page 67
immediately, the protocol can be safely stopped here. If you are
stopping, seal the ALP plate with a Microseal ‘B’ adhesive seal and store
at -15° to -25°C for up to seven days.
66
Part # 15026486 Rev. C
A single ‘A’ nucleotide is added to the 3’ ends of the blunt fragments to prevent them
from ligating to one another during the adapter ligation reaction. A corresponding
single ‘T’ nucleotide on the 3’ end of the adapter provides a complementary overhang
for ligating the adapter to the fragment. This strategy ensures a low rate of chimera
(concatenated template) formation.
Illumina-Supplied Consumables
} (Optional) A-Tailing Control (CTA) (1 tube per 48 reactions)
} A-Tailing Mix (ATL) (1 tube per 48 reactions)
} Resuspension Buffer (RSB) (1 tube)
User-Supplied Consumables
} Microseal ‘B’ Adhesive Seal
} RNase/DNase-free Reagent Reservoirs (if using multichannel pipettes)
} RNase/DNase-free Strip Tubes and Caps (if using multichannel pipettes)
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
• A-Tailing Mix
• A-Tailing Control
NOTE
The use of the A-Tailing Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Remove the ALP plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up IMP on page 64 and let stand to thaw at room temperature.
• Centrifuge the thawed ALP plate to 280 xg for 1 minute.
• Remove the adhesive seal from the ALP plate.
} Pre-heat the thermal cycler to 37°C.
} Choose the thermal cycler pre-heat lid option and set to 100°C
TruSeq DNA Sample Preparation Guide
67
Adenylate 3' Ends
Adenylate 3' Ends
Low Sample (LS) Protocol
Add ATL
1
Do one of the following:
• If using the in-line control reagent, add 2.5 µl of thawed A-Tailing Control to
each well of the ALP plate.
• If not using the in-line control reagent, add 2.5 µl of Resuspension Buffer to
each well of the ALP plate.
2
Add 12.5 µl of thawed A-Tailing Mix to each well of the ALP plate. Gently pipette
the entire volume up and down 10 times to mix thoroughly.
3
Seal the ALP plate with a Microseal ‘B’ adhesive seal.
Incubate 1 ALP
68
1
Place the sealed ALP plate on the pre-heated thermal cycler. Close the lid and
incubate at 37°C for 30 minutes.
2
Immediately remove the ALP plate from the thermal cycler, then proceed
immediately to Ligate Adapters on page 69.
Part # 15026486 Rev. C
This process ligates multiple indexing adapters to the ends of the DNA fragments,
preparing them for hybridization onto a flow cell.
Illumina-Supplied Consumables
} Ligation Mix (LIG) (1 tube per 48 reactions)
} Choose from the following depending on the kit you are using:
• TruSeq DNA LT Sample Prep Kit contents:
— DNA Adapter Indices (AD001–AD016, AD018–AD023, AD025, AD027)
(1 tube per column of 8 reactions, depending on the DNA Adapter Indices
being used)
• TruSeq DNA HT Sample Prep Kit contents:
— DAP (DNA Adapter Plate)
} (Optional) Ligation Control (CTL) (1 tube per 48 reactions)
} Resuspension Buffer (RSB) (1 tube)
} Stop Ligation Buffer (STL) (1 tube per 48 reactions)
} CAP (Clean Up ALP Plate) barcode label
} DAP (DNA Adapter Plate) barcode label (if using the HT kit)
} PCR (Polymerase Chain Reaction) barcode label (for gel-free method only)
} SSP (Size Separate Plate) barcode label (for gel method only)
User-Supplied Consumables
}
}
}
}
}
}
96-well 0.3 ml PCR plates (2)
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘B’ Adhesive Seals
RNase/DNase-free Reagent Reservoirs (if using multichannel pipettes)
RNase/DNase-free Strip Tubes and Caps (if using multichannel pipettes)
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
TruSeq DNA Sample Preparation Guide
69
Ligate Adapters
Ligate Adapters
Low Sample (LS) Protocol
• Appropriate DNA Adapter tubes (depending on the DNA Adapter Indices being
used) or the DAP.
— If using the DAP, review Handling Adapter Plate on page 42.
• Stop Ligation Buffer
NOTE
Do not remove the Ligation Mix tube from -15° to -25°C storage until
instructed to do so in the procedures.
} Remove the Ligation Control from -15° to -25°C storage and thaw it at room
temperature.
NOTE
The use of the Ligation Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Review Handling Magnetic Beads on page 12.
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Pre-heat the thermal cycler to 30°C.
} Choose the thermal cycler pre-heat lid option and set to 100°C
} Apply a CAP barcode label to a new 96-well 0.3 ml PCR plate.
} Do one of the following:
• If using the gel-free method, apply a PCR barcode label to a new 96-well
0.3 ml PCR plate.
• If using the gel method, apply a SSP barcode label to a new 96-well 0.3 ml PCR
plate.
NOTE
• When indexing libraries using adapter index tubes, Illumina recommends
arranging samples that will be combined into a common pool in the
same row. Each column should contain a common index. This will
facilitate pipetting operations when dispensing indexed adapters and
pooling indexed libraries later in the protocol.
• When indexing libraries with the DAP, arrange samples that will be
pooled together in the same orientation as the indices in the DAP.
NOTE
Illumina recommends that the DAP does not undergo more than 4
freeze/thaw cycles. To maximize the use of the DAP, process more than 24
samples at a time. These samples can then be pooled in any supported
configuration.
70
Part # 15026486 Rev. C
1
Do one of the following:
• If using DNA Adapter tubes, centrifuge the appropriate/desired thawed tubes to
600 xg for 5 seconds.
• If using a DAP:
— Thaw the plate for 10 minutes at room temperature on the benchtop.
Visually inspect the wells to ensure that they all are completely thawed.
— Remove the adapter plate tape seal.
— Centrifuge the plate at 280 xg for 1 minute to collect all of the adapter to the
bottom of the well.
— Remove the plastic cover and save the cover if you are not processing the
entire plate at once.
— If this is the first time using this DAP, apply the DAP barcode label to the
plate.
2
Centrifuge the Ligation Control (if using Ligation Control) and Stop Ligation Buffer
tubes to 600 xg for 5 seconds.
3
Immediately before use, remove the Ligation Mix tube from -15° to -25°C storage.
4
Remove the adhesive seal from the ALP plate.
5
Do one of the following:
• If using the in-line control reagent, add 2.5 µl of thawed Ligation Control to
each well of the ALP plate.
• If not using the in-line control reagent, add 2.5 µl of Resuspension Buffer to
each well of the ALP plate.
6
Add 2.5 µl of Ligation Mix to each well of the ALP plate.
7
Return the Ligation Mix tube back to -15° to -25°C storage immediately after use.
8
Do one of the following:
• If using DNA Adapter tubes, add 2.5 µl of the appropriate/desired thawed DNA
Adapter Index to each well of the ALP plate. Gently pipette the entire volume
up and down 10 times to mix thoroughly.
• If using a DAP:
TruSeq DNA Sample Preparation Guide
71
Ligate Adapters
Add LIG
Low Sample (LS) Protocol
— Place the DAP on the benchtop so that the part number barcode on the long
side of the plate is facing you and the clipped corner is located on the lower
left.
Figure 30 Correct DAP Orientation
— Do one of the following to pierce the foil seal:
— If using the entire plate at once, use the bottom of a clean 96-well semiskirted PCR plate to pierce a hole in all of the well seals simultaneously
by gently but firmly pressing the clean plate over the foil seal.
— If using only part of the plate, use the bottom of a clean eight-tube strip,
with caps attached, to pierce holes in the desired columns that will be
used for ligation. Repeat with a new, clean eight-tube strip, with caps
attached, for each column of adapters that will be used for ligation.
— Using an 8-tip multichannel pipette, transfer 2.5 µl of the
appropriate/desired thawed DNA Adapter from the DAP well to each well
of the ALP plate. Gently pipette the entire volume up and down 10 times to
mix thoroughly.
9
Seal the ALP plate with a Microseal ‘B’ adhesive seal.
10 Centrifuge the ALP plate to 280 xg for 1 minute.
Incubate 2 ALP
1
Incubate the ALP plate on the pre-heated thermal cycler, with the lid closed, at 30°C
for 10 minutes.
2
Remove the ALP plate from the thermal cycler.
1
Remove the adhesive seal from the ALP plate.
Add STL
72
Part # 15026486 Rev. C
Add 5 µl of Stop Ligation Buffer to each well of the ALP plate to inactivate the
ligation. Gently pipette the entire volume up and down 10 times to mix thoroughly.
Clean Up ALP
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
1
Vortex the AMPure XP Beads until they are well dispersed, then add 42.5 µl of
mixed AMPure XP Beads to each well of the ALP plate. Gently pipette the entire
volume up and down 10 times to mix thoroughly.
2
Incubate the ALP plate at room temperature for 15 minutes.
3
Place the ALP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
4
Remove and discard 80 µl of the supernatant from each well of the ALP plate.
NOTE
Leave the ALP plate on the magnetic stand while performing the following
80% EtOH wash steps (5–7).
5
With the ALP plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
6
Incubate the ALP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
7
Repeat steps 5 and 6 once for a total of two 80% EtOH washes.
8
While keeping the ALP plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes and then remove the plate from the magnetic stand.
9
Resuspend the dried pellet in each well with 52.5 µl Resuspension Buffer. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
10 Incubate the ALP plate at room temperature for 2 minutes.
11 Place the ALP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
TruSeq DNA Sample Preparation Guide
73
Ligate Adapters
2
Low Sample (LS) Protocol
12 Transfer 50 µl of the clear supernatant from each well of the ALP plate to the
corresponding well of the new 0.3 ml PCR plate labeled with the CAP barcode.
13 Vortex the AMPure XP Beads until they are well dispersed, then add 50 µl of mixed
AMPure XP Beads to each well of the CAP plate for a second clean up. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
14 Incubate the CAP plate at room temperature for 15 minutes.
15 Place the CAP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
16 Remove and discard 95 µl of the supernatant from each well of the CAP plate.
NOTE
Leave the CAP plate on the magnetic stand while performing the following
80% EtOH wash steps (17–19)
17 With the CAP plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
18 Incubate the CAP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
19 Repeat steps 17 and 18 once for a total of two 80% EtOH washes.
20 While keeping the CAP plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes and then remove the plate from the magnetic stand.
21 Resuspend the dried pellet in each well with 22.5 µl Resuspension Buffer. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
22 Incubate the CAP plate at room temperature for 2 minutes.
23 Place the CAP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
24 Do one of the following:
• If using the gel-free method:
— Transfer 20 µl of the clear supernatant from each well of the CAP plate to
the corresponding well of the new 0.3 ml PCR plate labeled with the PCR
barcode.
— Proceed to Enrich DNA Fragments on page 80.
• If using the gel method:
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Part # 15026486 Rev. C
SAFE STOPPING POINT
If you do not plan to proceed to Enrich DNA Fragments on page 80 or Purify
Ligation Products (gel method only) on page 76 immediately, the protocol can be
safely stopped here. If you are stopping, seal the PCR or SSP plate with a
Microseal ‘B’ adhesive seal and store at -15° to -25°C for up to seven days.
TruSeq DNA Sample Preparation Guide
75
Ligate Adapters
— Transfer 20 µl of the clear supernatant from each well of the CAP plate to
the corresponding well of the new 0.3 ml PCR plate labeled with the SSP
barcode.
— Proceed to Purify Ligation Products (gel method only) on page 76.
Low Sample (LS) Protocol
Purify Ligation Products (gel method only)
This process is only performed when using the gel method. If you are running the gelfree method in preparation for the TruSeq Enrichment protocol, proceed to Enrich DNA
Fragments on page 80.
NOTE
• TruSeq Enrichment refers to the Illumina TruSeq Exome Enrichment and
TruSeq Custom Enrichment Kits that can be used following TruSeq DNA
Sample Prep to prepare the library for sequencing targeted regions. For
more information, see the TruSeq Enrichment Guide.
• The gel-free method is not an option when preparing libraries for
standard (whole-genome) sequencing.
This process purifies the products of the ligation reaction on a gel and removes
unligated adapters, as well as any adapters that might have ligated to one another, and
selects a size-range of sequencing library appropriate for cluster generation.
Illumina suggests the following gel insert size targets and slice locations. The gel slice
locations account for the length of the adapter sequences flanking the inserts. For other
applications, other size ranges might be desired and the cut size adjusted accordingly.
Table 23 Size Selection Options
Insert Size Target
3 mm Slice Location
Whole-genome
Resequencing
300–400 bpa
400–500 bp
TruSeq Enrichment
200–300 bp
300–400 bp
a. +/- 1 standard deviation of 20 bp, i.e, a < 20% variance for read lengths of 2 × 75 bp or shorter
Illumina-Supplied Consumables
} PCR (Polymerase Chain Reaction Plate) barcode label
} Resuspension Buffer (RSB) (1 tube)
User-Supplied Consumables
} 50 X TAE Buffer
} 96-well 0.3 ml PCR plate
} BenchTop 100 bp DNA Ladder
76
Part # 15026486 Rev. C
Clean Scalpels
Certified Low-range Ultra Agarose
Distilled Water
6X Gel Loading Dye
MinElute Gel Extraction Kit
SyBr Gold Nucleic Acid Gel Stain
NOTE
Illumina strongly recommends using the user-supplied consumables
specified. Any deviation from these materials can result in incorrect sizeexcision or require additional user optimization.
Preparation
} Prepare 1X TAE buffer (> 1 L)
} Apply a PCR barcode label to a new 96-well 0.3 ml PCR plate.
} Remove the SSP plate from -15° to -25°C storage, if it was stored at the conclusion of
Clean Up ALP on page 73 and let stand to thaw at room temperature.
• Centrifuge the thawed SSP plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed SSP plate.
} Clean the tray, the comb, and the gel tank with ethanol and rinse them thoroughly
with deionized water to avoid cross contamination.
NOTE
Use the 12-well comb included with the recommended gel system.
Size Separate SSP
1
Prepare a 150 ml, 2% agarose with SyBr Gold gel using 1 X TAE Buffer as follows:
a Add 3 g of agarose powder in 150 ml of 1X TAE buffer.
b Microwave the gel buffer until the agarose powder is completely dissolved.
c Cool the gel buffer on the bench for 5 minutes, and then add 15 µl of SyBr Gold.
Swirl to mix.
d Pour the entire gel buffer to the gel tray.
NOTE
The final concentration of SyBr Gold should be 1X in the agarose gel buffer.
TruSeq DNA Sample Preparation Guide
77
Purify Ligation Products (gel method only)
}
}
}
}
}
}
Low Sample (LS) Protocol
WARNING
It is very important to pre-stain your gel with SyBr Gold. When using other
staining dyes or staining the gel after running, the DNA will migrate more
slowly than the ladder. This will result in cutting out the wrong size
fragments.
2
Remove the adhesive seal from the thawed SSP plate.
3
Add 4 µl of 6X Gel Loading Dye to each well of the SSP plate.
4
Add 17 µl Resuspension Buffer and 4 µl of 6X Gel Loading Dye to 3 µl of DNA
ladder.
WARNING
Do not to overload the DNA ladder. Without clear and distinct bands, it is
difficult to excise the correct fragment size. Also, an overloaded ladder might
run faster than the DNA sample library.
5
When the agarose gel is set, put it in the gel electrophoresis unit and fill the tank
with 1X TAE Buffer to the maximum fill mark.
Dimensions recommended for the electrophoresis unit;
12 cm x 14 cm (W x L), 800 ml buffer volume
6
Load all of the ladder solution onto one lane of the gel.
7
Load the samples from each well of the SSP plate onto the other lanes of the gel,
leaving a gap of at least one empty lane between samples and ladders.
NOTE
Flanking the library on both sides with ladders can make the library excision
easier.
NOTE
When handling multiple samples, to avoid the risk of cross-contamination
between libraries, leave a gap of at least one empty lane between samples
and use ladders on the first and last well of the gel to help locate the gel area
to be excised.
8
Run the gel at 120 V constant voltage for 120 minutes.
9
View the gel on a Dark Reader transilluminator.
10 Do one of the following:
78
Part # 15026486 Rev. C
NOTE
Cutting a band between 400–500 bp will result in an insert size of
approximately 300–400 bp, accounting for the size of the adapters. Adapters
add approximately 120 bp to each fragment. The sequencing read length
should be considered when cutting fragment sizes. Sequencing reads that
over-reach into the adapter will cause chimeric reads, unalignable to the
reference sequence.
NOTE
Use a clean scalpel per sample to avoid sample cross-contamination.
Size Separate Gel
1
Follow the instructions in the MinElute Gel Extraction Kit to purify each sample.
Incubate the gel slices in the QG solution at room temperature (not at 50°C as
instructed) until the gel slices have completely dissolved, while vortexing every
2 minutes.
2
Follow the instructions in the MinElute Gel Extraction Kit to purify on one
MinElute spin column, eluting in 25 µl of QIAGEN EB.
3
Transfer 20 µl of each sample from the MinElute collection tube to the new
0.3 ml PCR plate labeled with the PCR barcode using a single channel pipette.
SAFE STOPPING POINT
If you do not plan to proceed to Enrich DNA Fragments on page 80
immediately, the protocol can be safely stopped here. If you are
stopping, seal the PCR plate with a Microseal ‘B’ adhesive seal and store
at -15° to -25°C for up to seven days.
TruSeq DNA Sample Preparation Guide
79
Purify Ligation Products (gel method only)
• For whole-genome resequencing, excise a band from the gel spanning the width
of the lane and ranging in size from 400-500 bp using a clean scalpel. Use the
DNA ladder as a guide.
• For enrichment, excise a band from the gel spanning the width of the lane and
ranging in size from 300-400 bp using a clean scalpel. Use the DNA ladder as a
guide. For more information, see the TruSeq Enrichment Guide.
Low Sample (LS) Protocol
Enrich DNA Fragments
This process uses PCR to selectively enrich those DNA fragments that have adapter
molecules on both ends and to amplify the amount of DNA in the library. The PCR is
performed with a PCR primer cocktail that anneals to the ends of the adapters. The
number of PCR cycles should be minimized to avoid skewing the representation of the
library.
NOTE
PCR enriches for fragments that have adapters ligated on both ends.
Fragments with only one or no adapters on their ends are by-products of
inefficiencies in the ligation reaction. Neither species can be used to make
clusters, as fragments without any adapters cannot hybridize to surfacebound primers in the flow cell, and fragments with an adapter on only one
end can hybridize to surface bound primers but cannot form clusters.
Illumina-Supplied Consumables
}
}
}
}
PCR Master Mix (PMM) (1 tube per 48 reactions)
PCR Primer Cocktail (PPC) (1 tube per 48 reactions)
Resuspension Buffer (RSB) (1 tube)
TSP1 (Target Sample Plate) barcode label
User-Supplied Consumables
}
}
}
}
}
}
96-well 0.3 ml PCR plate
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘B’ Adhesive Seals
RNase/DNase-free Reagent Reservoirs (if using multichannel pipettes)
RNase/DNase-free Strip Tubes and Caps (if using multichannel pipettes)
Preparation
} Remove the PCR Master Mix and PCR Primer Cocktail from -15° to -25°C storage
and thaw them at room temperature. When thawed, keep the tubes on ice.
} Centrifuge the thawed PCR Master Mix and PCR Primer Cocktail tubes to 600 xg for
5 seconds.
} Review Handling Magnetic Beads on page 12.
80
Part # 15026486 Rev. C
NOTE
Illumina recommends 10 cycles of PCR for robust protocol performance.
However, to optimize yield versus cycle number, a titration of PCR cycles
can also be performed.
} Apply a TSP1 barcode label to a new 96-well 0.3 ml PCR plate.
Make PCR
The following procedure assumes 1 µg of input DNA to library preparation and is
designed to result in high library yields.
1
Add 5 µl of thawed PCR Primer Cocktail to each well of the PCR plate.
2
Add 25 µl of thawed PCR Master Mix to each well of the PCR plate. Gently pipette
the entire volume up and down 10 times to mix thoroughly.
3
Seal the PCR plate with a Microseal ‘B’ adhesive seal.
TruSeq DNA Sample Preparation Guide
81
Enrich DNA Fragments
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Remove the PCR plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up ALP on page 73 or Size Separate Gel on page 79 and let stand to thaw at
room temperature.
• Centrifuge the thawed PCR plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed PCR plate.
} Pre-program the thermal cycler with the following program and save as PCR:
• Choose the pre-heat lid option and set to 100°C
• 98°C for 30 seconds
• 10 cycles of:
— 98°C for 10 seconds
— 60°C for 30 seconds
— 72°C for 30 seconds
• 72°C for 5 minutes
• Hold at 10°C
Low Sample (LS) Protocol
Amp PCR
1
Place the sealed PCR plate on the pre-programmed thermal cycler. Close the lid and
select PCR to amplify the plate.
Clean Up PCR
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
1
Remove the adhesive seal from the PCR plate.
2
Vortex the AMPure XP Beads until they are well dispersed, then do one of the
following:
• If using the DNA Adapter tubes, add 50 µl of the mixed AMPure XP Beads to
each well of the PCR plate containing 50 µl of the PCR amplified library. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
• If using the DAP, add 47.5 µl of the mixed AMPure XP Beads to each well of
the PCR plate containing 50 µl of the PCR amplified library. Gently pipette the
entire volume up and down 10 times to mix thoroughly.
3
Incubate the PCR plate at room temperature for 15 minutes.
4
Place the PCR plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
5
Remove and discard 95 µl of the supernatant from each well of the PCR plate.
NOTE
Leave the PCR plate on the magnetic stand while performing the following
80% EtOH wash steps (6–8).
82
6
With the PCR plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
7
Incubate the PCR plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
8
Repeat steps 6 and 7 once for a total of two 80% EtOH washes.
Part # 15026486 Rev. C
While keeping the PCR plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes and then remove the plate from the magnetic stand.
10 Resuspend the dried pellet in each well with 32.5 µl Resuspension Buffer. Gently
pipette the entire volume up and down 10 times to mix thoroughly.
11 Incubate the PCR plate at room temperature for 2 minutes.
12 Place the PCR plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
13 Transfer 30 µl of the clear supernatant from each well of the PCR plate to the
corresponding well of the new 0.3 ml PCR plate labeled with the TSP1 barcode.
14 Do one of the following:
• If performing whole-genome resequencing, proceed to Validate Library on page
84.
• If performing enrichment, proceed to the TruSeq Enrichment Guide for
instructions on how to quantify and qualify your library.
SAFE STOPPING POINT
If you do not plan to proceed to Validate Library on page 84 or TruSeq
Enrichment immediately, the protocol can be safely stopped here. If you
are stopping, seal the TSP1 plate with a Microseal ‘B’ adhesive seal and
store at -15° to -25°C for up to seven days.
TruSeq DNA Sample Preparation Guide
83
Enrich DNA Fragments
9
Low Sample (LS) Protocol
Validate Library
Illumina recommends performing the following procedures for quality control analysis
on your whole-genome resequencing sample library and quantification of the DNA
library templates. If performing enrichment, proceed directly to the TruSeq Enrichment
Guide for instructions on how to quantify and qualify your library.
Quantify Libraries
In order to achieve the highest quality of data on Illumina sequencing platforms, it is
important to create optimum cluster densities across every lane of every flow cell. This
requires accurate quantitation of DNA library templates. Quantify your libraries using
qPCR according to the Illumina Sequencing Library qPCR Quantification Guide.
Quality Control (Optional)
To verify the size of your PCR enriched fragments, check the template size distribution
by running an aliquot of the DNA library on a gel or on a Agilent Technologies 2100
Bioanalyzer using a High Sensitivity DNA chip or DNA 1000 chip. Running samples
on a Bioanalyzer should be used for qualitative purposes only.
} If validating by gel, load 10% of the volume of the library on a gel and check that
the size range is as expected: a narrow smear similar in size to the DNA excised
from the gel after the ligation.
} If using the Agilent Bioanalyzer with a High Sensitivity DNA chip, make a 1:50
dilution of the library using water and load 1 µl of the diluted library on the Agilent
High Sensitivity DNA chip.
} If using the Agilent Bioanalyzer with a DNA 1000 chip, load 1 µl of the library on
the Agilent DNA 1000 chip.
84
Part # 15026486 Rev. C
Figure 32 DNA PCR Product
NOTE
For a gel size selected library, if the DNA is not a narrow smear, but is
comprised of a long smear of several hundred base pairs, or contains an
intense 126 bp fragment (adapter-dimer), then another purification step is
recommended. Repeat Purify Ligation Products (gel method only) on page 76.
TruSeq DNA Sample Preparation Guide
85
Validate Library
Figure 31 Example of DNA Library Size Distribution for Whole-Genome Resequencing
Low Sample (LS) Protocol
Figure 33 Example of DNA Library Size Distribution with the Gel-Free Method
86
Part # 15026486 Rev. C
This process describes how to prepare DNA templates that will be applied to cluster
generation. Indexed DNA libraries are normalized to 10 nM in the DCT plate and then
pooled in equal volumes in the PDP plate. DNA libraries not intended for indexing are
normalized to 10 nM in the DCT plate without pooling.
Illumina-Supplied Consumables
} DCT (Diluted Cluster Template) barcode label
} PDP (Pooled DCT Plate) barcode label (for indexing only)
User-Supplied Consumables
}
}
}
}
96-well 0.3 ml PCR plate (for indexing only)
96-well MIDI plate
Microseal ‘B’ Adhesive seals
Tris-Cl 10 mM, pH8.5 with 0.1% Tween 20
Preparation
} Apply a DCT barcode label to a new 96-well MIDI plate.
} Apply a PDP barcode label to a new 96-well 0.3 ml PCR plate (for indexing only).
} Remove the TSP1 plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up PCR on page 82, and let stand to thaw at room temperature.
• Centrifuge the thawed TSP1 plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed TSP1 plate.
Make DCT
1
Transfer 10 µl of sample library from each well of the TSP1 plate to the
corresponding well of the new MIDI plate labeled with the DCT barcode.
2
Normalize the concentration of sample library in each well of DCT plate to 10 nM
using Tris-Cl 10 mM, pH 8.5 with 0.1% Tween 20.
NOTE
Depending on the yield quantification data of each sample library, the final
volume in the DCT plate can vary from 10-400 µl.
TruSeq DNA Sample Preparation Guide
87
Normalize and Pool Libraries
Normalize and Pool Libraries
Low Sample (LS) Protocol
3
Gently pipette the entire normalized sample library volume up and down 10 times
to mix thoroughly.
4
Depending on the type of library you want to generate, do one of the following:
• For non-indexed libraries, the protocol stops here. Do one of the following:
— Proceed to cluster generation. For more information, see the Illumina Cluster
Generation User Guide.
— Seal the DCT plate with a Microseal ‘B’ adhesive seal and store at -15° to
-25°C.
• For indexed libraries, proceed to Make PDP.
Make PDP (for indexing only)
NOTE
Do not make a PDP plate if there is no pooling.
1
Determine the number of samples to be combined together for each pool.
NOTE
Keep track of which sample goes into which well, to avoid pooling two
samples with the same index.
2
88
Do one of the following:
• If pooling 2–24 samples:
— Transfer 10 µl of each normalized sample library to be pooled from the
DCT plate to one well of the new 0.3 ml PCR plate labeled with the PDP
barcode.
The total volume in each well of the PDP plate should be 10X the number of
combined sample libraries and will be 20–240 µl (2–24 libraries). For example,
the volume for 2 samples is 20 µl, the volume for 12 samples is 120 µl, or the
volume for 24 samples is 240 µl.
• If pooling 25–96 samples:
— Using a multichannel pipette, transfer 5 µl of each normalized sample
library in column 1 from the DCT plate to column 1 of the new MIDI plate
labeled with the PDP barcode.
— Transfer 5 µl of each normalized sample library in column 2 from the DCT
plate to column 1 of the PDP plate.
Part # 15026486 Rev. C
3
Gently pipette the entire volume up and down 10 times to mix thoroughly.
4
Do one of the following:
• Proceed to cluster generation. For more information, see the Illumina Cluster
Generation User Guide.
• Seal the PDP plate with a Microseal ‘B’ adhesive seal and store at -15° to -25°C.
TruSeq DNA Sample Preparation Guide
89
Normalize and Pool Libraries
— Repeat the transfer for as many times as there are remaining columns in the
DCT plate. The result will be a PDP plate with pooled samples in column 1.
Gently pipette the entire volume of each well of column 1 up and down 10
times to mix thoroughly.
— Combine the contents of each well of column 1 into well A2 of the PDP
plate, for the final pool.
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Part # 15026486 Rev. C
Chapter 4 High Sample (HS) Protocol
Introduction
Sample Prep Workflow
Fragment DNA
Perform End Repair
Adenylate 3' Ends
Ligate Adapters
Purify Ligation Products (gel method only)
Enrich DNA Fragments
Validate Library
Normalize and Pool Libraries
TruSeq DNA Sample Preparation Guide
92
94
95
99
103
105
112
116
120
123
91
Chapter 4
High Sample (HS) Protocol
High Sample (HS) Protocol
Introduction
This chapter describes the TruSeq DNA Sample Preparation high sample (HS) protocol.
Illumina recommends the following kit, sample number, and protocol combinations:
Table 24 Kit and Sample Number Recommendations
Number of Samples
Processed
At One Time
Kit
Recommended
<24
LT
24–48
LT or HT
>48
HT
Table 25 Kit and Protocol Recommendations
Kit
Number of
Samples
Supported
Number of Samples
Processed
At One Time
Protocol
LT
48
≤48
LS
>48
HS
≤48
LS
>48
HS
HT
96
} Review Best Practices on page 11 before proceeding.
} Follow the protocols in the order shown, using the specified volumes and
incubation parameters.
} This HS protocol requires shaking and heating equipment to mix reagents and for
incubation (see Consumables and Equipment on page 32).
} For optimal sample tracking and quality control, fill out the Lab Tracking Form as
you perform the sample preparation. For more information, see Tracking Tools on
page 26.
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Part # 15026486 Rev. C
TruSeq DNA Sample Preparation Guide
93
Introduction
} If you are pooling using adapter index tubes, record information about your
samples before beginning library preparation for later use in data analysis. For more
information, see Tracking Tools on page 26. Illumina recommends arranging
samples that will be combined into a common pool in the same row. Each column
should contain a common index. This will facilitate pipetting operations when
dispensing indexed adapters and pooling indexed libraries later in the protocol.
} If you are pooling with the DAP, review the planning steps in Pooling Preparation
with Adapter Plate on page 41 before beginning library preparation.
High Sample (HS) Protocol
Sample Prep Workflow
The following figure illustrates the processes of the TruSeq DNA Sample Preparation HS
protocol to prepare templates using 24 indexed adapter tubes or a DAP.
Figure 34 TruSeq DNA Sample Preparation HS Workflow
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Part # 15026486 Rev. C
This process describes how to optimally fragment the gDNA depending on the
downstream application. Covaris shearing generates dsDNA fragments with 3' or 5'
overhangs. The fragmentation process described below was optimized to obtain final
libraries with the following differences:
Table 26 Fragmentation Method Options
Whole-genome
Resequencing
Gel Method
Covaris Shearing
Duration
Insert Size
40 seconds
300–400 bp
TruSeq Enrichment
Gel-free
Gel Method
Method
120 seconds
100–900 bp
200–300 bp
NOTE
If fragmenting using a nebulization technique, skip this procedure and
perform the Appendix A Alternate Fragmentation Protocols. The
nebulization procedures have only been validated for whole-genome
resequencing or enrichment with the gel-method.
Calculate the amount of DNA to be fragmented based on 1 µg input DNA for each
sample.
Illumina-Supplied Consumables
}
}
}
}
Resuspension Buffer (RSB) (1 tube)
CFP (Covaris Fragmentation Plate) barcode label
DNA (DNA Plate) barcode label
IMP (Insert Modification Plate) barcode label
User-Supplied Consumables
} 96-well MIDI plates (2)
} Covaris Tubes
} DNA samples
TruSeq DNA Sample Preparation Guide
95
Fragment DNA
Fragment DNA
High Sample (HS) Protocol
Preparation
} Review DNA Input Recommendations on page 22.
} Remove one tube of Resuspension Buffer from -15° to -25°C storage and thaw it at
room temperature.
NOTE
The Resuspension Buffer can be stored at 2° to 8°C after the initial thaw.
} Turn on the Covaris instrument at least 30 minutes before starting.
• Following the manufacturer’s instructions, de-gas and pre-chill the water to a
temperature of 3° to 6°C. You can start the fragmentation procedure at 6°C.
} Apply a CFP barcode label to the Covaris tube plate.
} Apply a DNA barcode label to a new 96-well MIDI plate.
} Apply a IMP barcode label to a new 96-well MIDI plate.
Make CFP
1
Illumina recommends to quantify gDNA samples using a fluorometric-based
method such as Qubit or PicoGreen.
2
Illumina recommends to normalize the gDNA samples to a final volume of 55 µl at
20 ng/µl into each well of the new MIDI plate labeled with the DNA barcode.
Fragment DNA
1
Shear 1 µg of gDNA sample by transferring 52.5 µl of each DNA sample from the
DNA plate to each Covaris tube in the new HSP plate labeled with CFP barcode.
NOTE
Load the DNA sample into the Covaris tube very slowly to avoid creating
air bubbles. However, air bubbles might not be preventable during the
process run.
2
96
Fragment the DNA using the following settings:
Part # 15026486 Rev. C
Fragment DNA
Table 27 Covaris S220 or Covaris E220 Settings
Whole-genome
Resequencing
TruSeq Enrichment
Duty factor
10%
10%
Peak Incident
Power
175
175
Cycles per burst
200
200
40 seconds
2 x 60 seconds
(120 seconds total)
Frequency sweeping
Frequency
sweeping
5.5° to 6°C
5.5° to 6°C
Setting
Duration
Mode
Temperature
Table 28 Covaris S2 or E210 Settings
Whole-genome
Resequencing
TruSeq Enrichment
Duty cycle
10%
10%
Intensity
5.0
5.0
Cycles per
burst
200
200
40 seconds
2 x 60 seconds
(120 seconds total)
Frequency sweeping
Frequency
sweeping
Covaris S2 - 23W
Covaris E210 - 18W
Covaris S2 - 23W
Covaris E210 - 18W
5.5° to 6°C
5.5° to 6°C
Setting
Duration
Mode
Displayed
Power
Temperature
3
Seal the Covaris tubes and centrifuge to 600 xg for 1 minute.
TruSeq DNA Sample Preparation Guide
97
High Sample (HS) Protocol
4
Transfer 50 µl of fragmented DNA from each Covaris tube in the CFP plate to the
corresponding well of the new MIDI plate labeled with the IMP barcode using a
single channel pipette.
NOTE
• When indexing libraries using adapter index tubes, Illumina recommends
arranging samples that will be combined into a common pool in the
same row. Each column should contain a common index. This will
facilitate pipetting operations when dispensing indexed adapters and
pooling indexed libraries later in the protocol.
• When indexing libraries with the DAP, arrange samples that will be
pooled together in the same orientation as the indices in the DAP.
98
Part # 15026486 Rev. C
This process converts the overhangs resulting from fragmentation into blunt ends using
an End Repair Mix. The 3' to 5' exonuclease activity of this mix removes the 3'
overhangs and the polymerase activity fills in the 5' overhangs.
Illumina-Supplied Consumables
}
}
}
}
(Optional) End Repair Control (CTE) (1 tube per 48 reactions)
End Repair Mix (ERP) (1 tube per 48 reactions)
Resuspension Buffer (RSB) (1 tube)
ALP (Adapter Ligation Plate) barcode label
User-Supplied Consumables
}
}
}
}
}
}
}
96-well MIDI plate
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘B’ Adhesive Seal
PCR Grade Water (for gel-free method only)
RNase/DNase-free Reagent Reservoirs
RNase/DNase-free Strip Tubes and Caps
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
• End Repair Control
• End Repair Mix
NOTE
The use of the End Repair Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Review Handling Magnetic Beads on page 12.
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Pre-heat the microheating system to 30°C.
} Calibrate the microplate shaker with a stroboscope and set it to 1,800 rpm.
TruSeq DNA Sample Preparation Guide
99
Perform End Repair
Perform End Repair
High Sample (HS) Protocol
} Apply a ALP barcode label to a new 96-well MIDI plate.
Make IMP
1
Do one of the following:
• If using the in-line control reagent:
— Centrifuge the thawed End Repair Control tube to 600 xg for 5 seconds.
— Add 10 µl of thawed End Repair Control to each well of the IMP plate that
contains 50 µl of fragmented DNA.
• If not using the in-line control reagent, add 10 µl of Resuspension Buffer to each
well of the IMP plate that contains 50 µl of fragmented DNA.
2
Add 40 µl of End Repair Mix to each well of the IMP plate containing the
fragmented DNA. Mix thoroughly as follows:
a Seal the IMP plate with a Microseal ‘B’ adhesive seal.
b Shake the IMP plate on a microplate shaker at 1,800 rpm for 2 minutes.
c Centrifuge the IMP plate to 280 xg for 1 minute.
Incubate 1 IMP
1
Place the sealed IMP plate on the pre-heated microheating system. Close the lid and
incubate at 30°C for 30 minutes.
2
Remove the IMP plate from the microheating system.
Clean Up IMP
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
100
1
Remove the adhesive seal from the IMP plate.
2
Vortex the AMPure XP Beads until they are well dispersed.
3
Do one of the following:
• If using the gel-free method for enrichment:
— Determine the amount of AMPure XP beads and PCR grade water needed
to combine to prepare a diluted bead mixture:
AMPure XP beads: # of samples X 160 µl x 0.85 = µl AMPure XP beads. For
Part # 15026486 Rev. C
4
Mix thoroughly as follows:
a Seal the IMP plate with a Microseal ‘B’ adhesive seal.
b Shake the IMP plate on a microplate shaker at 1,800 rpm for 2 minutes.
5
Incubate the IMP plate at room temperature for 15 minutes.
6
Place the IMP plate on the magnetic stand at room temperature for 15 minutes or
until the liquid appears clear.
7
Remove the adhesive seal from the IMP plate.
8
Using a 200 µl single channel or multichannel pipette set to 127.5 µl, remove and
discard 127.5 µl of the supernatant from each well of the IMP plate.
9
Repeat step 8 once.
NOTE
Leave the IMP plate on the magnetic stand while performing the following
80% EtOH wash steps (10–12).
10 With the IMP plate on the magnetic stand, add 200 µl of freshly prepared 80%
EtOH to each well with a sample without disturbing the beads.
11 Incubate the IMP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
12 Repeat steps 10 and 11 once for a total of two 80% EtOH washes.
13 Let the IMP plate stand at room temperature for 15 minutes to dry, then remove the
plate from the magnetic stand.
14 Resuspend the dried pellet in each well with 17.5 µl Resuspension Buffer. Mix
thoroughly as follows:
a Seal the IMP plate with a Microseal ‘B’ adhesive seal.
b Shake the IMP plate on a microplate shaker at 1,800 rpm for 2 minutes.
TruSeq DNA Sample Preparation Guide
101
Perform End Repair
example, 6.528 ml of AMPure XP beads are needed for 48 samples.
PCR grade water: # of samples X 160 µl x 0.15 = µl PCR grade water. For
example, 1.152 ml of PCR grade water is needed for 48 samples.
— Add 160 µl of the diluted bead mixture to each well of the IMP plate
containing 100 µl of End Repair Mix.
• If using the gel method, add 160 µl well-mixed AMPure XP Beads to each well
of the IMP plate containing 100 µl of End Repair Mix.
High Sample (HS) Protocol
c
Centrifuge the IMP plate to 280 xg for 1 minute.
15 Incubate the IMP plate at room temperature for 2 minutes.
16 Place the IMP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
17 Remove the adhesive seal from the IMP plate.
18 Transfer 15 µl of the clear supernatant from each well of the IMP plate to the
corresponding well of the new MIDI plate labeled with the ALP barcode.
SAFE STOPPING POINT
If you do not plan to proceed to Adenylate 3' Ends on page 103
immediately, the protocol can be safely stopped here. If you are
stopping, seal the ALP plate with a Microseal ‘B’ adhesive seal and store
at -15° to -25°C for up to seven days.
102
Part # 15026486 Rev. C
A single ‘A’ nucleotide is added to the 3’ ends of the blunt fragments to prevent them
from ligating to one another during the adapter ligation reaction. A corresponding
single ‘T’ nucleotide on the 3’ end of the adapter provides a complementary overhang
for ligating the adapter to the fragment. This strategy ensures a low rate of chimera
(concatenated template) formation.
Illumina-Supplied Consumables
} (Optional) A-Tailing Control (CTA) (1 tube per 48 reactions)
} A-Tailing Mix (ATL) (1 tube per 48 reactions)
} Resuspension Buffer (RSB) (1 tube)
User-Supplied Consumables
} Microseal ‘B’ Adhesive Seal
} RNase/DNase-free Reagent Reservoirs
} RNase/DNase-free Strip Tubes and Caps
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
• A-Tailing Mix
• A-Tailing Control
NOTE
The use of the A-Tailing Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Remove the ALP plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up IMP on page 100 and let stand to thaw at room temperature.
• Centrifuge the thawed ALP plate to 280 xg for 1 minute
• Remove the adhesive seal from the ALP plate.
} Pre-heat the microheating system to 37°C.
TruSeq DNA Sample Preparation Guide
103
Adenylate 3' Ends
Adenylate 3' Ends
High Sample (HS) Protocol
Add ATL
1
Do one of the following:
• If using the in-line control reagent, add 2.5 µl of thawed A-Tailing Control to
each well of the ALP plate.
• If not using the in-line control reagent, add 2.5 µl of Resuspension Buffer to
each well of the ALP plate.
2
Add 12.5 µl of thawed A-Tailing Mix to each well of the ALP plate. Mix thoroughly
as follows:
a Seal the ALP plate with a Microseal ‘B’ adhesive seal.
b Shake the ALP plate on a microplate shaker at 1,800 rpm for 2 minutes.
c Centrifuge the ALP plate to 280 xg for 1 minute.
Incubate 1 ALP
104
1
Place the sealed ALP plate on the pre-heated microheating system. Close the lid and
incubate at 37°C for 30 minutes.
2
Immediately remove the ALP plate from the microheating system, then proceed
immediately to Ligate Adapters on page 105.
Part # 15026486 Rev. C
This process ligates indexing adapters to the ends of the DNA fragments, preparing
them for hybridization onto a flow cell.
Illumina-Supplied Consumables
} Ligation Mix (LIG) (1 tube per 48 reactions)
} Choose from the following depending on the kit you are using:
• TruSeq DNA LT Sample Prep Kit contents:
— DNA Adapter Indices (AD001–AD016, AD018–AD023, AD025, AD027)
(1 tube per column of 8 reactions, depending on the DNA Adapter Indices
being used)
• TruSeq DNA HT Sample Prep Kit contents:
— DAP (DNA Adapter Plate)
} (Optional) Ligation Control (CTL) (1 tube per 48 reactions)
} Resuspension Buffer (RSB) (1 tube)
} Stop Ligation Buffer (STL) (1 tube per 48 reactions)
} CAP (Clean Up ALP Plate) barcode label
} DAP (DNA Adapter Plate) barcode label (if using the HT kit)
} PCR (Polymerase Chain Reaction) barcode label (for gel-free method only)
} SSP (Size Separate Plate) barcode label (for gel method only)
User-Supplied Consumables
}
}
}
}
}
}
}
96-well MIDI plate
96-well HSP plate
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘B’ Adhesive Seals
RNase/DNase-free Reagent Reservoirs
RNase/DNase-free Strip Tubes and Caps
Preparation
} Remove the following from -15° to -25°C storage and thaw them at room
temperature:
TruSeq DNA Sample Preparation Guide
105
Ligate Adapters
Ligate Adapters
High Sample (HS) Protocol
• Appropriate DNA Adapter tubes (depending on the DNA Adapter Indices being
used) or the DAP.
— If using the DAP, review Handling Adapter Plate on page 42.
• Stop Ligation Buffer
NOTE
Do not remove the Ligation Mix tube from -15° to -25°C storage until
instructed to do so in the procedures.
} Remove the Ligation Control from -15° to -25°C storage and thaw it at room
temperature.
NOTE
The use of the Ligation Control is optional and it can be replaced with the
same volume of Resuspension Buffer.
} Review Handling Magnetic Beads on page 12.
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Pre-heat the microheating system 1 to 30°C.
} Apply a CAP barcode label to a new 96-well MIDI plate.
} Do one of the following:
• If using the gel-free method for enrichment, apply a PCR barcode label to a new
96-well HSP plate.
• If using the gel method, apply a SSP barcode label to a new 96-well HSP plate.
NOTE
• When indexing libraries using adapter index tubes, Illumina recommends
arranging samples that will be combined into a common pool in the
same row. Each column should contain a common index. This will
facilitate pipetting operations when dispensing indexed adapters and
pooling indexed libraries later in the protocol.
• When indexing libraries with the DAP, arrange samples that will be
pooled together in the same orientation as the indices in the DAP.
NOTE
Illumina recommends that the DAP does not undergo more than 4
freeze/thaw cycles. To maximize the use of the DAP, process more than 24
samples at a time. These samples can then be pooled in any supported
configuration.
106
Part # 15026486 Rev. C
1
Do one of the following:
• If using DNA Adapter tubes, centrifuge the appropriate/desired thawed tubes to
600 xg for 5 seconds.
• If using a DAP:
— Thaw the plate for 10 minutes at room temperature on the benchtop.
Visually inspect the wells to ensure that they all are completely thawed.
— Remove the adapter plate tape seal.
— Centrifuge the plate at 280 xg for 1 minute to collect all of the adapter to the
bottom of the well.
— Remove the plastic cover and save the cover if you are not processing the
entire plate at once.
— If this is the first time using this DAP, apply the DAP barcode label to the
plate.
2
Centrifuge the Ligation Control (if using Ligation Control) and Stop Ligation Buffer
tubes to 600 xg for 5 seconds.
3
Immediately before use, remove the Ligation Mix tube from -15° to -25°C storage.
4
Remove the adhesive seal from the ALP plate.
5
Do one of the following:
• If using the in-line control reagent, add 2.5 µl of thawed Ligation Control to
each well of the ALP plate.
• If not using the in-line control reagent, add 2.5 µl of Resuspension Buffer to
each well of the ALP plate.
6
Add 2.5 µl of Ligation Mix to each well of the ALP plate.
7
Return the Ligation Mix tube back to -15° to -25°C storage immediately after use.
8
Do one of the following:
• If using DNA Adapter tubes, add 2.5 µl of the appropriate/desired thawed DNA
Adapter Index to each well of the ALP plate.
• If using a DAP:
TruSeq DNA Sample Preparation Guide
107
Ligate Adapters
Add LIG
High Sample (HS) Protocol
— Place the DAP on the benchtop so that the part number barcode on the long
side of the plate is facing you and the clipped corner is located on the lower
left.
Figure 35 Correct DAP Orientation
— Do one of the following to pierce the foil seal:
— If using the entire plate at once, use the bottom of a clean 96-well semiskirted PCR plate to pierce a hole in all of the well seals simultaneously
by gently but firmly pressing the clean plate over the foil seal.
— If using only part of the plate, use the bottom of a clean eight-tube strip,
with caps attached, to pierce holes in the desired columns that will be
used for ligation. Repeat with a new, clean eight-tube strip, with caps
attached, for each column of adapters that will be used for ligation.
— Using an 8-tip multichannel pipette, transfer 2.5 µl of the
appropriate/desired thawed DNA Adapter from the DAP well to each well
of the ALP plate.
9
Mix thoroughly as follows:
a Seal the ALP plate with a Microseal ‘B’ adhesive seal.
b Shake the ALP plate on a microplate shaker at 1,800 rpm for 2 minutes.
c Centrifuge the ALP plate to 280 xg for 1 minute.
Incubate 2 ALP
108
1
Incubate the ALP plate on the pre-heated microheating system, with the lid closed,
at 30°C for 10 minutes.
2
Remove the ALP plate from the microheating system.
Part # 15026486 Rev. C
1
Remove the adhesive seal from the ALP plate.
2
Add 5 µl of Stop Ligation Buffer to each well of the ALP plate to inactivate the
ligation mix. Mix thoroughly as follows:
a Seal the ALP plate with a Microseal ‘B’ adhesive seal.
b Shake the ALP plate on a microplate shaker at 1,800 rpm for 2 minutes.
c Centrifuge the ALP plate to 280 xg for 1 minute.
Clean Up ALP
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
1
Remove the adhesive seal from the ALP plate.
2
Vortex the AMPure XP Beads until they are well dispersed, then add 42.5 µl of
mixed AMPure XP Beads to each well of the ALP plate. Mix thoroughly as follows:
a Seal the ALP plate with a Microseal ‘B’ adhesive seal.
b Shake the ALP plate on a microplate shaker at 1,800 rpm for 2 minutes.
3
Incubate the ALP plate at room temperature for 15 minutes.
4
Place the ALP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
5
Remove the adhesive seal from the ALP plate.
6
Remove and discard 80 µl of the supernatant from each well of the ALP plate.
NOTE
Leave the ALP plate on the magnetic stand while performing the following
80% EtOH wash steps (7–9).
7
With the ALP plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
8
Incubate the ALP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
9
Repeat steps 7 and 8 once for a total of two 80% EtOH washes.
TruSeq DNA Sample Preparation Guide
109
Ligate Adapters
Add STL
High Sample (HS) Protocol
10 While keeping the ALP plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes.
11 Resuspend the dried pellet in each well with 52.5 µl Resuspension Buffer. Mix
thoroughly as follows:
a Seal the ALP plate with a Microseal ‘B’ adhesive seal.
b Shake the ALP plate on a microplate shaker at 1,800 rpm for 2 minutes.
12 Incubate the ALP plate at room temperature for 2 minutes.
13 Place the ALP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
14 Remove the adhesive seal from the ALP plate.
15 Transfer 50 µl of the clear supernatant from each well of the ALP plate to the
corresponding well of the new MIDI plate labeled with the CAP barcode.
16 Vortex the AMPure XP Beads until they are well dispersed, then add 50 µl of mixed
AMPure XP Beads to each well of the CAP plate. Mix thoroughly as follows:
a Seal the CAP plate with a Microseal ‘B’ adhesive seal.
b Shake the CAP plate on a microplate shaker at 1,800 rpm for 2 minutes.
17 Incubate the CAP plate at room temperature for 15 minutes.
18 Place the CAP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
19 Remove the adhesive seal from the CAP plate.
20 Remove and discard 95 µl of the supernatant from each well of the CAP plate.
NOTE
Leave the CAP plate on the magnetic stand while performing the following
80% EtOH wash steps (21–23)
21 With the CAP plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
22 Incubate the CAP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
23 Repeat steps 21 and 22 once for a total of two 80% EtOH washes.
110
Part # 15026486 Rev. C
25 Resuspend the dried pellet in each well with 22.5 µl Resuspension Buffer. Mix
thoroughly as follows:
a Seal the CAP plate with a Microseal ‘B’ adhesive seal.
b Shake the CAP plate on a microplate shaker at 1,800 rpm for 2 minutes.
26 Incubate the CAP plate at room temperature for 2 minutes.
27 Place the CAP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
28 Remove the adhesive seal from the CAP plate.
29 Do one of the following:
• If using the gel-free method for enrichment:
— Transfer 20 µl of the clear supernatant from each well of the CAP plate to
the corresponding well of the new HSP plate labeled with the PCR barcode.
— Proceed to Enrich DNA Fragments on page 116.
• If using the gel method:
— Transfer 20 µl of the clear supernatant from each well of the CAP plate to
the corresponding well of the new HSP plate labeled with the SSP barcode.
— Proceed to Purify Ligation Products (gel method only) on page 112.
SAFE STOPPING POINT
If you do not plan to proceed to Enrich DNA Fragments on page 116 or
Purify Ligation Products (gel method only) on page 112 immediately, the
protocol can be safely stopped here. If you are stopping, seal the PCR or
SSP plate with a Microseal ‘B’ adhesive seal and store at -15° to -25°C for
up to seven days.
TruSeq DNA Sample Preparation Guide
111
Ligate Adapters
24 While keeping the CAP plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes.
High Sample (HS) Protocol
Purify Ligation Products (gel method only)
This process is only performed when using the gel method. If you are running the gelfree method in preparation for the TruSeq Enrichment protocol, proceed to Enrich DNA
Fragments on page 116.
NOTE
• TruSeq Enrichment refers to the Illumina TruSeq Exome Enrichment and
TruSeq Custom Enrichment Kits that can be used following TruSeq DNA
Sample Prep to prepare the library for sequencing targeted regions. For
more information, see the TruSeq Enrichment Guide.
• The gel-free method is not an option when preparing libraries for
standard (whole-genome) sequencing.
This process purifies the products of the ligation reaction on a gel and removes
unligated adapters, as well as any adapters that might have ligated to one another, and
selects a size-range of sequencing library appropriate for cluster generation.
Illumina suggests the following gel insert size targets and slice locations. The gel slice
locations account for the length of the adapter sequences flanking the inserts. For other
applications, other size ranges might be desired and the cut size adjusted accordingly.
Table 29 Size Selection Options
Insert Size Target
3 mm Slice Location
Whole-genome
Resequencing
300–400 bpa
400–500 bp
TruSeq Enrichment
200–300 bp
300–400 bp
a. +/- 1 standard deviation of 20 bp, i.e, a < 20% variance for read lengths of 2 × 75 bp or shorter
Illumina-Supplied Consumables
} PCR (Polymerase Chain Reaction Plate) barcode label
} Resuspension Buffer (RSB) (1 tube)
User-Supplied Consumables
} 50 X TAE Buffer
} 96-well HSP plate
} BenchTop 100 bp DNA Ladder
112
Part # 15026486 Rev. C
Clean Scalpels
Certified Low-range Ultra Agarose
Distilled Water
6X Gel Loading Dye
MinElute Gel Extraction Kit
SyBr Gold Nucleic Acid Gel Stain
NOTE
Illumina strongly recommends using the user-supplied consumables
specified. Any deviation from these materials can result in incorrect sizeexcision or require additional user optimization
Preparation
} Prepare 1X TAE buffer (> 1 L)
} Apply a PCR barcode label to a new 96-well HSP plate.
} Remove the SSP plate from -15° to -25°C storage, if it was stored at the conclusion of
Clean Up ALP on page 109 and let stand to thaw at room temperature.
• Centrifuge the thawed SSP plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed SSP plate.
} Clean the tray, the comb, and the gel tank with ethanol and rinse them thoroughly
with deionized water to avoid cross contamination.
NOTE
Use the 12-well comb included with the recommended gel system.
Size Separate SSP
1
Prepare a 150 ml, 2% agarose with SyBr Gold gel using 1 X TAE Buffer as follows:
a Add 3 g of agarose powder in 150 ml of 1X TAE buffer.
b Microwave the gel buffer until the agarose powder is completely dissolved.
c Cool the gel buffer on the bench for 5 minutes, and then add 15 µl of SyBr Gold.
Swirl to mix.
d Pour the entire gel buffer to the gel tray.
NOTE
The final concentration of SyBr Gold should be 1X in the agarose gel buffer.
TruSeq DNA Sample Preparation Guide
113
Purify Ligation Products (gel method only)
}
}
}
}
}
}
High Sample (HS) Protocol
WARNING
It is very important to pre-stain your gel with SyBr Gold. When using other
staining dyes or staining the gel after running, the DNA will migrate more
slowly than the ladder. This will result in cutting out the wrong size
fragments.
2
Remove the adhesive seal from the thawed SSP plate.
3
Add 4 µl of 6X Gel Loading Dye to each well of the SSP plate.
4
Add 17 µl Resuspension Buffer and 4 µl of 6X Gel Loading Dye to 3 µl of DNA
ladder.
WARNING
Do not to overload the DNA ladder. Without clear and distinct bands, it is
difficult to excise the correct fragment size. Also, an overloaded ladder might
run faster than the DNA sample library.
5
When the agarose gel is set, put it in the gel electrophoresis unit and fill the tank
with 1X TAE Buffer to the maximum fill mark.
Dimensions recommended for the electrophoresis unit;
12 cm x 14 cm (W x L), 800 ml buffer volume
6
Load all of the ladder solution onto one lane of the gel.
7
Load the samples from each well of the SSP plate onto the other lanes of the gel,
leaving a gap of at least one empty lane between samples and ladders.
NOTE
Flanking the library on both sides with ladders can make the library excision
easier.
NOTE
When handling multiple samples, to avoid the risk of cross-contamination
between libraries, leave a gap of at least one empty lane between samples
and use ladders on the first and last well of the gel to help locate the gel area
to be excised.
8
Run the gel at 120 V constant voltage for 120 minutes.
9
View the gel on a Dark Reader transilluminator.
10 Do one of the following:
114
Part # 15026486 Rev. C
NOTE
Cutting a band between 400–500 bp will result in an insert size of
approximately 300–400 bp, accounting for the size of the adapters. Adapters
add approximately 120 bp to each fragment. The sequencing read length
should be considered when cutting fragment sizes. Sequencing reads that
over-reach into the adapter will cause chimeric reads, unalignable to the
reference sequence.
NOTE
Use a clean scalpel per sample to avoid sample cross-contamination.
Size Separate Gel
1
Follow the instructions in the MinElute Gel Extraction Kit to purify each sample.
Incubate the gel slices in the QG solution at room temperature (not at 50°C as
instructed) until the gel slices have completely dissolved, while vortexing every
2 minutes.
2
Follow the instructions in the MinElute Gel Extraction Kit to purify on one
MinElute spin column, eluting in 25 µl of QIAGEN EB.
3
Transfer 20 µl of each sample from the MinElute collection tube to the new
HSP plate labeled with the PCR barcode using a single channel pipette.
SAFE STOPPING POINT
If you do not plan to proceed to Enrich DNA Fragments on page 116
immediately, the protocol can be safely stopped here. If you are
stopping, seal the PCR plate with a Microseal ‘B’ adhesive seal and store
at -15° to -25°C for up to seven days.
TruSeq DNA Sample Preparation Guide
115
Purify Ligation Products (gel method only)
• For whole-genome resequencing, excise a band from the gel spanning the width
of the lane and ranging in size from 400-500 bp using a clean scalpel. Use the
DNA ladder as a guide.
• For enrichment, excise a band from the gel spanning the width of the lane and
ranging in size from 300-400 bp using a clean scalpel. Use the DNA ladder as a
guide. For more information, see the TruSeq Enrichment Guide.
High Sample (HS) Protocol
Enrich DNA Fragments
This process uses PCR to selectively enrich those DNA fragments that have adapter
molecules on both ends and to amplify the amount of DNA in the library. The PCR is
performed with a PCR primer cocktail that anneals to the ends of the adapters. The
number of PCR cycles should be minimized to avoid skewing the representation of the
library.
NOTE
PCR enriches for fragments that have adapters ligated on both ends.
Fragments with only one or no adapters on their ends are by-products of
inefficiencies in the ligation reaction. Neither species can be used to make
clusters, as fragments without any adapters cannot hybridize to surfacebound primers in the flow cell, and fragments with an adapter on only one
end can hybridize to surface bound primers but cannot form clusters.
Illumina-Supplied Consumables
}
}
}
}
}
PCR Master Mix (PMM) (1 tube per 48 reactions)
PCR Primer Cocktail (PPC) (1 tube per 48 reactions)
Resuspension Buffer (RSB) (1 tube)
CPP (Clean Up PCR Plate) barcode label
TSP1 (Target Sample Plate) barcode label
User-Supplied Consumables
}
}
}
}
}
}
}
}
96-well MIDI plate
96-well HSP plate
AMPure XP Beads
Freshly Prepared 80% Ethanol (EtOH)
Microseal ‘A’ Film
Microseal ‘B’ Adhesive Seals
RNase/DNase-free Reagent Reservoirs
RNase/DNase-free Strip Tubes and Caps
Preparation
} Remove the PCR Master Mix and PCR Primer Cocktail from -15° to -25°C storage
and thaw them at room temperature. When thawed, keep the tubes on ice.
116
Part # 15026486 Rev. C
NOTE
Illumina recommends 10 cycles of PCR for robust protocol performance.
However, to optimize yield versus cycle number, a titration of PCR cycles
can also be performed.
} Apply a CPP barcode label to a new 96-well MIDI plate.
} Apply a TSP1 barcode label to a new 96-well HSP plate.
Make PCR
The following procedure assumes 1 µg of input DNA to library preparation and is
designed to result in high library yields.
1
Add 5 µl of thawed PCR Primer Cocktail to each well of the PCR plate.
2
Add 25 µl of thawed PCR Master Mix to each well of the PCR plate. Mix
thoroughly as follows:
a Seal the PCR plate with a Microseal ‘A’ film.
TruSeq DNA Sample Preparation Guide
117
Enrich DNA Fragments
} Centrifuge the thawed PCR Master Mix and PCR Primer Cocktail tubes to 600 xg for
5 seconds.
} Review Handling Magnetic Beads on page 12.
} Remove the AMPure XP beads from storage and let stand for at least 30 minutes to
bring them to room temperature.
} Remove the PCR plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up ALP on page 109 or Size Separate Gel on page 115 and let stand to thaw
at room temperature.
• Centrifuge the thawed PCR plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed PCR plate.
} Pre-program the thermal cycler with the following program and save as PCR:
• Choose the pre-heat lid option and set to 100°C
• 98°C for 30 seconds
• 10 cycles of:
— 98°C for 10 seconds
— 60°C for 30 seconds
— 72°C for 30 seconds
• 72°C for 5 minutes
• Hold at 10°C
High Sample (HS) Protocol
WARNING
Follow the vendor's instructions for applying Microseal "A" sealing films.
Improper use could lead to inefficient sealing (evaporation of sample or
cross contamination) or too efficient sealing (parts of the seal remain in the
well after removing the whole seal).
b
c
Shake the PCR plate on a microplate shaker at 1,600 rpm for 20 seconds.
Centrifuge the PCR plate to 280 xg for 1 minute.
Amp PCR
1
Place the sealed PCR plate on the pre-programmed thermal cycler. Close the lid and
select PCR to amplify the plate.
Clean Up PCR
NOTE
Before performing clean up, review Handling Magnetic Beads on page 12
when working with AMPure XP Beads.
118
1
Remove the adhesive seal from the PCR plate.
2
Vortex the AMPure XP Beads until they are well dispersed, then do one of the
following:
• If using the DNA Adapter tubes, add 50 µl of the mixed AMPure XP Beads to
each well of the new MIDI plate labeled with the CPP barcode.
• If using the DAP, add 47.5 µl of the mixed AMPure XP Beads to each well of
the new MIDI plate labeled with the CPP barcode.
3
Transfer the entire contents from each well of the PCR plate to the corresponding
well of the CPP plate containing 50 µl of mixed AMPure XP Beads. Mix thoroughly
as follows:
a Seal the CPP plate with a Microseal ‘B’ adhesive seal.
b Shake the CPP plate on a microplate shaker at 1,800 rpm for 2 minutes.
4
Incubate the CPP plate at room temperature for 15 minutes.
5
Place the CPP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
6
Remove the adhesive seal from the CPP plate.
Part # 15026486 Rev. C
Remove and discard 95 µl of the supernatant from each well of the CPP plate.
NOTE
Leave the CPP plate on the magnetic stand while performing the following
80% EtOH wash steps (8–10).
8
With the CPP plate remaining on the magnetic stand, add 200 µl of freshly
prepared 80% EtOH to each well without disturbing the beads.
9
Incubate the CPP plate at room temperature for 30 seconds, then remove and
discard all of the supernatant from each well.
10 Repeat steps 8 and 9 once for a total of two 80% EtOH washes.
11 While keeping the CPP plate on the magnetic stand, let the samples air dry at room
temperature for 15 minutes.
12 Resuspend the dried pellet in each well with 32.5 µl Resuspension Buffer. Mix
thoroughly as follows:
a Seal the CPP plate with a Microseal ‘B’ adhesive seal.
b Shake the CPP plate on a microplate shaker at 1,800 rpm for 2 minutes.
13 Incubate the CPP plate at room temperature for 2 minutes.
14 Place the CPP plate on the magnetic stand at room temperature for 5 minutes or
until the liquid appears clear.
15 Remove the adhesive seal from the CPP plate.
16 Transfer 30 µl of the clear supernatant from each well of the CPP plate to the
corresponding well of the new HSP plate labeled with the TSP1 barcode.
17 Do one of the following:
• If performing whole-genome resequencing, proceed to Validate Library on page
120.
• If performing enrichment, proceed to the TruSeq Enrichment Guide for
instructions on how to quantify and qualify your library.
SAFE STOPPING POINT
If you do not plan to proceed to Validate Library on page 120 or TruSeq
Enrichment immediately, the protocol can be safely stopped here. If you
are stopping, seal the TSP1 plate with a Microseal ‘B’ adhesive seal and
store at -15° to -25°C for up to seven days.
TruSeq DNA Sample Preparation Guide
119
Enrich DNA Fragments
7
High Sample (HS) Protocol
Validate Library
Illumina recommends performing the following procedures for quality control analysis
on your whole-genome resequencing sample library and quantification of the DNA
library templates. If performing enrichment, proceed directly to the TruSeq Enrichment
Guide for instructions on how to quantify and qualify your library.
Quantify Libraries
In order to achieve the highest quality of data on Illumina sequencing platforms, it is
important to create optimum cluster densities across every lane of every flow cell. This
requires accurate quantitation of DNA library templates. Quantify your libraries using
qPCR according to the Illumina Sequencing Library qPCR Quantification Guide.
Quality Control (Optional)
To verify the size of your PCR enriched fragments, check the template size distribution
by running an aliquot of the DNA library on a gel or on a Agilent Technologies 2100
Bioanalyzer using a High Sensitivity DNA chip or DNA 1000 chip. Running samples
on a Bioanalyzer should be used for qualitative purposes only.
} If validating by gel, load 10% of the volume of the library on a gel and check that
the size range is as expected: a narrow smear similar in size to the DNA excised
from the gel after the ligation.
} If using the Agilent Bioanalyzer with a High Sensitivity DNA chip, make a 1:50
dilution of the library using water and load 1 µl of the diluted library on the Agilent
High Sensitivity DNA chip.
} If using the Agilent Bioanalyzer with a DNA 1000 chip, load 1 µl of the library on
the Agilent DNA 1000 chip.
120
Part # 15026486 Rev. C
Figure 37 DNA PCR Product
NOTE
For a gel size selected library, if the DNA is not a narrow smear, but is
comprised of a long smear of several hundred base pairs, or contains an
intense 126 bp fragment (adapter-dimer), then another purification step is
recommended. Repeat Purify Ligation Products (gel method only) on page 112.
TruSeq DNA Sample Preparation Guide
121
Validate Library
Figure 36 Example of DNA Library Size Distribution for Whole-Genome Resequencing
High Sample (HS) Protocol
Figure 38 Example of DNA Library Size Distribution with the Gel-Free Method
122
Part # 15026486 Rev. C
This process describes how to prepare DNA templates that will be applied to cluster
generation. Indexed DNA libraries are normalized to 10 nM in the DCT plate and then
pooled in equal volumes in the PDP plate. DNA libraries not intended for indexing are
normalized to 10 nM in the DCT plate without pooling.
Illumina-Supplied Consumables
} DCT (Diluted Cluster Template) barcode label
} PDP (Pooled DCT Plate) barcode label (for indexing only)
User-Supplied Consumables
}
}
}
}
96-well HSP plate (for indexing only)
96-well MIDI plate
Microseal ‘B’ Adhesive seals
Tris-Cl 10 mM, pH8.5 with 0.1% Tween 20
Preparation
} Apply a DCT barcode label to a new 96-well MIDI plate.
} Apply a PDP barcode label to a new 96-well HSP plate (for indexing only).
} Remove the TSP1 plate from -15° to -25°C storage, if it was stored at the conclusion
of Clean Up PCR on page 118, and let stand to thaw at room temperature.
• Centrifuge the thawed TSP1 plate to 280 xg for 1 minute.
• Remove the adhesive seal from the thawed TSP1 plate.
Make DCT
1
Transfer 10 µl of sample library from each well of the TSP1 plate to the
corresponding well of the new MIDI plate labeled with the DCT barcode.
2
Normalize the concentration of sample library in each well of DCT plate to 10 nM
using Tris-Cl 10 mM, pH 8.5 with 0.1% Tween 20.
NOTE
Depending on the yield quantification data of each sample library, the final
volume in the DCT plate can vary from 10-400 µl.
TruSeq DNA Sample Preparation Guide
123
Normalize and Pool Libraries
Normalize and Pool Libraries
High Sample (HS) Protocol
3
Mix the DCT plate as follows:
a Seal the DCT plate with a Microseal ‘B’ adhesive seal.
b Shake the DCT plate on a microplate shaker at 1,000 rpm for 2 minutes.
c Centrifuge the DCT plate to 280 xg for 1 minute.
d Remove the adhesive seal from the DCT plate.
4
Depending on the type of library you want to generate, do one of the following:
• For non-indexed libraries, the protocol stops here. Do one of the following:
— Proceed to cluster generation. For more information, see the Illumina Cluster
Generation User Guide.
— Seal the DCT plate with a Microseal ‘B’ adhesive seal and store at -15° to
-25°C.
• For indexed libraries, proceed to Make PDP.
Make PDP (for indexing only)
NOTE
Do not make a PDP plate if there is no pooling.
1
Determine the number of samples to be combined together for each pool.
NOTE
Keep track of which sample goes into which well, to avoid pooling two
samples with the same index.
2
124
Do one of the following:
• If pooling 2–24 samples:
— Transfer 10 µl of each normalized sample library to be pooled from the
DCT plate to one well of the new 0.3 ml PCR plate labeled with the PDP
barcode.
The total volume in each well of the PDP plate should be 10X the number of
combined sample libraries and will be 20–240 µl (2–24 libraries). For example,
the volume for 2 samples is 20 µl, the volume for 12 samples is 120 µl, or the
volume for 24 samples is 240 µl.
• If pooling 25–96 samples:
— Using a multichannel pipette, transfer 5 µl of each normalized sample
library in column 1 from the DCT plate to column 1 of the new MIDI
labeled with the PDP barcode.
Part # 15026486 Rev. C
3
Mix the PDP plate as follows:
a Seal the PDP plate with a Microseal ‘B’ adhesive seal.
b Shake the PDP plate on a microplate shaker at 1,800 rpm for 2 minutes.
4
Do one of the following:
• Proceed to cluster generation. For more information, see the Illumina Cluster
Generation User Guide.
• Seal the PDP plate with a Microseal ‘B’ adhesive seal and store at -15° to -25°C.
TruSeq DNA Sample Preparation Guide
125
Normalize and Pool Libraries
— Transfer 5 µl of each normalized sample library in column 2 from the DCT
plate to column 1 of the PDP plate.
— Repeat the transfer for as many times as there are remaining columns in the
DCT plate. The result will be a PDP plate with pooled samples in column 1.
Mix the PDP plate as follows:
— Seal PDP plate with Microseal ‘B’ adhesive seal.
— Shake PDP plate on microplate shaker at 1,800 rpm for 2 minutes.
— Combine the contents of each well of column 1 into well A2 of the PDP
plate, for the final pool.
126
Part # 15026486 Rev. C
Appendix A Alternate Fragmentation Protocols
Introduction
Procedure
TruSeq DNA Sample Preparation Guide
128
129
127
Appendix A
Alternate Fragmentation
Protocols
Alternate Fragmentation Protocols
Introduction
An alternative fragmentation method for TruSeq DNA Sample Preparation to the
procedures described in Fragment DNA on page 59 for the LS protocol or Fragment DNA
on page 95 for the HS protocol is using a nebulization technique, which breaks up DNA
into pieces less than 800 bp in minutes using a disposable device. This process
generates double-stranded DNA fragments containing 3' or 5' overhangs.
NOTE
These nebulization procedures have only been validated for whole-genome
resequencing or enrichment with the gel-method.
Illumina-Supplied Consumables
} IMP (Insert Modification Plate) barcode label
User-Supplied Consumables
} 96-well 0.3 ml PCR plate (for LS protocol), or
} 96-well MIDI plate (for HS protocol)
} The following consumables are provided in the Paired-End Sample Preparation Kit:
• Nebulizers (box of 10 nebulizers and vinyl accessory tubes)
• Nebulization Buffer (7 ml)
• TE Buffer
} QIAquick PCR Purification Kit
} Purified DNA (0.1–2 µg, 2 µg recommended)
DNA should be as intact as possible, with an OD260/280 ratio of 1.8–2.0
} Compressed Air of at least 32 psi
Do not use CO which could alter the pH of the nebulizer buffer
2
} PVC tubing
Dimensions: 1/4 inch ID, 3/8 inch OD, 1/16 inch wall, 1 meter length
128
Part # 15026486 Rev. C
The DNA sample to be processed should be highly pure, having an
OD260/280 ratio of between 1.8 and 2.0, and should be as intact as possible.
NOTE
If you are not familiar with this shearing method, Illumina recommends that
you test this procedure on test samples and practice assembling the
nebulizer before proceeding with your sample DNA.
1
Remove a nebulizer from the plastic packaging and unscrew the blue lid.
Figure 39 Remove the Nebulizer Lid
2
Using gloves, remove a piece of vinyl tubing from the packaging and slip it over
the central atomizer tube. Push it all the way to the inner surface of the blue lid.
Figure 40 Assemble the Nebulizer
A
B
C
Blue Lid
Atomizer
Vinyl Tubing
TruSeq DNA Sample Preparation Guide
129
Procedure
Procedure
Alternate Fragmentation Protocols
3
Add 0.1–2 µg of Purified DNA in a total volume of 50 µl of TE Buffer to the
nebulizer.
4
Add 700 µl Nebulization Buffer to the DNA and mix well.
5
Screw the lid back on (finger-tight).
Figure 41 Replace the Nebulizer Lid
6
Chill the nebulizer containing the DNA solution on ice while performing the next
step.
7
Connect the compressed air source to the inlet port on the top of the nebulizer with
the PVC tubing, ensuring a tight fit.
Figure 42 Connect Compressed Air
130
8
Bury the nebulizer in an ice bucket and place it in a fume hood.
9
Use the regulator on the compressed air source to make sure the air is delivered at
32-35 psi.
Part # 15026486 Rev. C
11 Centrifuge the nebulizer at 450 xg for 2 minutes to collect the droplets from the side
of the nebulizer. If necessary, use an old nebulizer as a counter-balance.
12 If a centrifuge is not available, then use 2 ml of the binding buffer (PB or PBI buffer)
from the QIAquick PCR Purification Kit to rinse the sides of the nebulizer and
collect the DNA solution at the base of the nebulizer.
13 Measure the recovered volume. Typically, you should recover 400–600 µl.
14 Follow the instructions in the QIAquick PCR Purification Kit to purify the sample
solution and concentrate it on one QIAquick column, eluting in 50 µl of QIAGEN
EB.
15 Transfer all of the 50 µl of fragmented DNA to each well of the new plate labeled
with the IMP barcode using a single channel pipette.
16 Do one of the following:
• For LS processing, proceed to Perform End Repair on page 63.
• For HS processing, proceed to Perform End Repair on page 99.
SAFE STOPPING POINT
If you do not plan to proceed to Perform End Repair immediately, the
protocol can be safely stopped here. If you are stopping, store the
samples at -15° to -25°C overnight or longer. When proceeding, thaw
the samples on ice.
TruSeq DNA Sample Preparation Guide
131
Procedure
10 Nebulize for 6 minutes. You might notice vapor rising from the nebulizer; this is
normal. Also, the Nebulization Buffer might turn white or appear frozen.
132
Part # 15026486 Rev. C
5
50 X TAE Buffer 76, 112
6
6X gel loading dye 77, 113
A
Acronyms 9
Add ATL 68, 104
Add LIG 71
Add STL 72, 109
Agilent Bioanalyzer 11
ALP 63, 99
Amp PCR 82, 118
AMPure XP Beads iii, 12, 63, 69, 80,
99, 105, 116
ATL 67, 103
B
BenchTop 100 bp DNA ladder 76,
112
C
CAP 69, 105
certified low-range ultra agarose 77,
113
CFP 59, 95
Clean Up ALP 73, 109
Clean Up IMP 64, 100
Clean Up PCR v, 82, 118
cluster generation 2, 89, 125
contamination 14
Covaris instrument 60, 96
TruSeq DNA Sample Preparation Guide
Index
Index
Covaris shearing iv, 5, 59, 95
Covaris tubes 59, 95
cross-contamination 14
CTA 67, 103
CTE 63, 99
CTL 69, 105
customer support 137
D
DAP iii, iv, 14, 16, 41-42, 69, 105
DCT 87, 123
DNA Adapter Indices 69, 105
DNA PCR product 84, 120
DNA Plate (DNA) 59, 95
DNA sequencing 2
documentation 137
dsDNA 11, 128
E
ERP 63, 99
experienced user card (EUC) 26
Experiment Manager iv, 26, 45-46,
50
F
Fragment DNA 60, 96
fragmentation 128
G
gDNA 2
gel-free method 2, 64, 100
gel insert size 5, 59, 95
gel method 5, 65, 101
133
Index
H
P
help, technical 137
High Sample (HS) iii, 4
High Throughput (HT) iii
HSP 4
paired-end 2
PCR 3, 69, 76, 105, 112
PCR grade water 63, 99
PDP 87, 123
PMM v, 80, 116
pooled sample volumes 88, 124
pooling 41-42, 45
PPC iv, v, 80, 116
purified DNA 128
I
IMP 59, 64, 95, 100, 128
in-line control DNA 24
Incubate 1 ALP 68, 104
Incubate 1 IMP 64, 100
indexed adapter 37-38
L
lab tracking form (LTF) 26
LIG 69, 105
liquid handling 11
Low Sample (LS) 4
Low Throughput (LT) iii
M
magnetic beads 12
Make CFP 60, 96
Make DCT 87, 123
Make IMP 64, 100
Make PCR v, 81, 117
Make PDP v, 88, 124
master-mixed reagents 2
micro plate shaker 4
microheating system 4
MIDI 4
MinElute Gel Extraction Kit 77, 113
N
nebulization 128
nebulizer 128
normalize gDNA 60, 96
134
Q
QIAquick PCR Purification Kit 128
qPCR 11
quality control 84, 120
quantify libraries 84, 120
quantitation 22
quantity and quality 22
R
Reagent reservoirs 63, 67, 69, 80, 99,
103, 105, 116
RSB 59, 63, 67, 69, 76, 95, 99, 103,
105, 112, 116
S
sample sheet iv
SAV 24-25
shear gDNA 60, 96
shearing 2
single read 2
Size Separate Gel 79, 115
Size Separate SSP 77, 113
SSP 69, 105
STL 69, 105
strip tubes and caps 63, 67, 69, 80,
99, 103, 105, 116
SyBr Gold gel stain 77, 113
Part # 15026486 Rev. C
Index
T
TE buffer 128
technical assistance 137
temperature 14
thermal cycler 4, 21
Tris-Cl 87, 123
TruSeq Enrichment 3, 5, 59, 76, 95,
112
TSP1 80, 87, 116, 123
U
Usage Guidelines iii, 15
W
whole-genome resequencing 3, 5, 59,
76, 95, 112
workflow diagram 58, 94
TruSeq DNA Sample Preparation Guide
135
Index
136
Part # 15026486 Rev. C
For technical assistance, contact Illumina Customer Support.
Table 30 Illumina General Contact Information
Illumina Website
Email
http://www.illumina.com
[email protected]
Table 31 Illumina Customer Support Telephone Numbers
Region
Contact Number
Region
Contact Number
North America
1.800.809.4566
Italy
800.874909
Austria
0800.296575
Netherlands
0800.0223859
Belgium
0800.81102
Norway
800.16836
Denmark
80882346
Spain
900.812168
Finland
0800.918363
Sweden
020790181
France
0800.911850
Switzerland
0800.563118
Germany
0800.180.8994
United Kingdom
0800.917.0041
Ireland
1.800.812949
Other countries
+44.1799.534000
MSDSs
Material safety data sheets (MSDSs) are available on the Illumina website at
http://www.illumina.com/msds.
Product Documentation
You can obtain PDFs of additional product documentation from the Illumina website.
Go to http://www.illumina.com/support and select a product. To download
documentation, you will be asked to log in to MyIllumina. After you log in, you can
view or save the PDF. To register for a MyIllumina account, please visit
https://my.illumina.com/Account/Register.
TruSeq DNA Sample Preparation Guide
137
Technical Assistance
Technical Assistance
Illumina
Headquartered in San Diego, California, U.S.A.
+1.800.809.ILMN (4566)
+1.858.202.4566 (outside North America)
[email protected]
www.illumina.com
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