This is a protocol for generating RAD libraries for Illumina sequencing. With this technique, 96 samples can be multiplexed into one sequencing library, and only tags adjacent to PstI sites are sequenced. This is a cheap way to both mine and genotype large numbers of SNPs. This is the protocol developed in Erik Sacks' lab at UIUC by Lindsay Clark, based on protocols from Pat Brown and Megan Hall.
- Quant-iT Picogreen kit (Invitrogen)
- Qiagen gel purification kit
- Qiagen PCR cleanup kit
- From New England Biolabs:
- PstI-HF, 20,000 U/mL
- MspI, 20,000 U/mL
- T4 DNA ligase, 2,000,000 U/mL
- Phusion High Fidelity PCR master mix
- 100 bp DNA ladder
- gel loading dye that does NOT have bromophenol blue
Note: MspI is not a heat-inactivated enzyme, but I have found that the protocol works anyway. Between the ligation and gel extraction steps, I keep the sample on ice to prevent any residual digestion activity.
- You will also need a black microtiter plate for the Picogreen assay.
This is the most expensive part of the protocol other than the sequencing itself, since 192 oligonucleotides must be ordered.
Adapter 1 top:
Adapter 1 bottom:
yyyy are the barcode and its reverse complement, respectively.
Barcodes and oligo sequences are from Pat Brown's lab.
Illumina PCR primers:
- Nanodrop spectrophotometer
- BioTek Synergy plate reader (for reading fluorescence)
- Ordinary PCR machine
- Agarose gel rig
- real-time PCR machine (we just pay the core facility to do that part)
Top and bottom strands of adapters need to be annealed 1X Annealing Buffer, which is 10 mM Tris, 50 mM NaCl.
The annealing program is:
- 95°C 5 minutes
- Ramp down -0.1°C every 2 seconds (or -1°C every 20 seconds) to 25°C.
- Pat Brown provided us with a plate of PstI adapters that are at 1 μM. I took a bottle of autoclaved 1X Annealing Buffer, added 45 μl to each well of a 96-well plate, then transferred 5 μl from the 1 μM plate to make a 0.1 μM working stock.
- MspI adapters are ordered like normal oligos, and I have 100 μM concentrated stocks in TE. To make a 10 μM stock:
- 20 μl A2top, 100 μM
- 20 μl A2bot, 100 μM
- 20 μl 500 mM NaCl
- 2 μl 1M Tris
- 138 μl nuclease-free water
- Mix well, add 100 μl to each of two PCR tubes, and run them on the annealing program ("Adapt" on the PCR machine).
DNA quantification and dilution
- Quantify your DNA using the Nanodrop spectrophotometer.
- If the DNA concentration is greater than 200 ng/ul, dilute to 200 ng/ul. I find it useful to set up these dilutions on a 96-well plate. If the DNA is between 50 and 200 ng/ul, just put an aliquot directly on your dilution plate. If it is less than 50 ng/ul, you need to redo the extraction or find a way to concentrate the DNA.
Quantify your ≤200 ng/ul dilution plate using Picogreen:
- Take the tube of bright orange Picogreen reagent out ahead of time to thaw. Wrap it in aluminum foil to protect it from light. It is in DMSO instead of water, so it takes a long time to thaw and will immediately freeze solid if you put it on ice.
- The Quant-iT Picogreen kit comes with a lambda DNA standard at 100 ug/ml. Dilute some of the 20X TE that comes with the kit to 1X TE, and use it to make a 2 ug/ml dilution of the lambda DNA. (1:50 dilution.)
- For one plate (88 samples, 8 standards) make up 20 mL of 1X TE. (1 mL of the TE that comes with the kit, plus 19 mL sterilized filtered water.)
- The plate you need for the assay is a black, flat-well plastic plate. (Corning makes these.)
- Set up a standard curve in column 1 (or column 12, doesn’t matter). Pipette 100 ul of TE into wells B-H. Add 100 ul of your 2 ug/ml lambda standard each to well A and B. Pipette well B up and down to mix, then transfer 100 ul to well C. Pipette well C up and down to mix, then transfer 100 ul to well D. Continue through well G, and leave well H as a blank. (After mixing well G, you will simply throw out 100 ul.)
- Add 99 ul TE to the other 88 (or however many samples you are doing) wells . Add 1 ul of ≤200 ng/ul sample DNA to each well.
- Add 50 ul of Quant-iT reagent to 10 mL of 1X TE. This solution needs to be used within a few hours, even if it is protected from light. Add 100 ul of the solution to each well (both sample, standard, and blank).
- Picogreen bonded to dsDNA has an excitation maximum at 480 nm and emission maximum at 520 nm. The plate readers in IGB (BioTek Synergy HT) probably already have a picogreen program on them.
- Read fluorescence intensity on the plate reader, and export it to Microsoft Excel.
- Make a scatterplot of fluorescence intensity of the standard vs. the standard concentration. Given that the samples were diluted 200X, the standard concentration is multiplied by 200:
- Well A 200 ng/ul
- Well B 100
- Well C 50
- Well D 25
- Well E 12.5
- Well F 6.25
- Well G 3.125
- Well H 0
- In Excel, fit a trendline to the scatterplot and display the equation on the chart. Use this equation to estimate the concentration of the samples.
In most cases, the concentration estimate via Picogreen should be lower than the concentration estimate via Nanodrop. This is because Nanodrop measures DNA + RNA, whereas Picogreen only measures DNA. Why didn’t we just use Picogreen to begin with? Because it can measure a much narrower range of concentrations than Nanodrop can. If the standard curve were any more concentrated, it would not be linear.
Based on the Picogreen concentration estimates, dilute the DNA to 50 ng/μL in 10 mM Tris (and 0.1 mM EDTA, optional).
Restriction digestion and ligation
Restriction digestion master mix:
|Ingredient||For one sample||For one plate|
|50 ng/ul DNA||5 ul||-|
|10X NEBuffer 4||1.5 ul||165 ul|
|PstI-HF, 20,000 U/mL||0.25 ul||27.5 ul|
|MspI, 20,000 U/mL||0.25 ul||27.5 ul|
|Nuclease-free water||8 ul||880 ul|
(I have also used DNA at a concentration of 100 ng/ul because that was what Keck wanted for GoldenGate, so then I used 2.5 ul DNA and 10.5 ul water.)
Do this in a 96-well plate. Pipette the DNA into the wells and then add 10 ul of master mix to everything. Pick one well that will not have DNA in it. This will be an important control later on to demonstrate that this library was not contaminated with another library (which will have a different empty well).
Run the Digest program on the PCR machine: 3 hours at 37°C, then 20 minutes at 80°C.
Using a multichannel pipette, add 2.5 μL of 0.1 μM PstI adapters to their corresponding wells on the digestion plate. (Do add the adapter corresponding to the well that has no DNA in it.)
Ligation master mix, keep on ice until use:
|Ingredient||For one sample||For one plate|
|10X Ligase buffer with ATP||1 ul||100 ul|
|10 μM MspI adapter||0.5 ul||55 ul|
|10 mM ATP||1.5 ul||165 ul|
|T4 Ligase, 2M U/mL||0.1 ul||11 ul|
|Nuclease-free water||5.4 ul||594 ul|
Add 8.5 μL of ligation master mix to each well of the digestion plate.
Run on the "ligate" program on the PCR machine: 2 hours at 25°C, 20 minutes at 65°C.
Cleanup and amplification
- Using a multichannel pipette and a PCR 8-well strip tube, pool all the columns together, adding 5 μL from each well of the plate to the wells on the strip tube.
- Pipette the 60 μL out of each well on the strip tube into one 1.5 mL tube. Mix well so that all samples are combined evenly. Freeze or keep on ice.
- Pour a 2% agarose gel with ethidium bromide. Make it nice and deep; my recipe is 3 g agarose, 150 mL 1X TAE, and 7.5 μL ethidium bromide solution. Use a wide-toothed comb.
- Take 40 μL (or more depending on your well volume) of your pooled library and combine it with a loading dye that does not have bromophenol blue. I actually use 10 μL of Promega GoTaq Green PCR buffer, despite the fact that I'm not doing PCR, since it doubles as a loading dye and lacks bromophenol blue.
- I recommend cleaning out your gel rig and putting in fresh TAE, since you especially want to avoid any contamination from other Illumina libraries.
- Run your ~50 μL of library plus loading dye on the gel. The lane with the library should have a lane of 100 bp ladder on either side of it. You can put multiple libraries on one gel, but leave several empty lanes between them.
- The gel doesn't need to be run very long. I would go 20 minutes at 100 V, or until the ladder bands below 500 bp are distinguishable.
- The library should look like a smear. There may be some undigested DNA (a band in the 10's of kb) but that is okay as long as most of the DNA is digested. There may also be a thick band of leftover adapter below 100 bp.
- Using a clean razor blade for each library, cut out the smear between 200 bp and 500 bp. There should definitely be DNA visible in this range.
- Use the Qiagen gel extraction kit to purify the DNA out of this gel slice. Elute in the lower volume (30 μL EB).
- Run the Illumina PCR:
- 3 μL gel-extracted library
- 2 μL 10 μM forward + reverse Illumina primers (PCR1 and PCR2)
- 25 μL 2X Phusion Master mix
- 20 μL nuclease-free water
- PCR program:
- 98°C 30 seconds
- 15 cycles of 98°C 10 seconds, 65°C 30 seconds, 72°C 30 seconds
- 72°C 5 minutes
- Use the Qiagen PCR cleanup kit to purify the amplified library. Elute in 50 μL EB.
Please feel free to post comments, questions, or improvements to this protocol. Happy to have your input!
- List troubleshooting tips here.
- You can also link to FAQs/tips provided by other sources such as the manufacturer or other websites.
- Anecdotal observations that might be of use to others can also be posted here.
Please sign your name to your note by adding '''*~~~~''': to the beginning of your tip.
- Elshire RJ, Glaubitz JC, Sun Q, Poland JA, Kawamoto K, Buckler ES, and Mitchell SE (2011) "A robust, simple Genotyping-by-Sequencing (GBS) approach for high diversity species." PLoS One 6(5): e19379. doi:10.1371/journal.pone.0019379
- Who has experience with this protocol?
or instead, discuss this protocol.