- What you’ll need
- Cell Preparation
- Transposition Reaction and Purification
- PCR Amplification
- Purification of Final RNA-Seq Library Using AMPure Beads
- Quality Check of Final Product
- Sequencing Guidelines
- Normalize and Pool
- Setup Run in Basespace
- Loading the Sequencer
Assay for Transposase Accessible Chromatin (ATAC-seq) has been shown to be compatible with many methods for cell collection and has also worked effectively across many cell types and species. However, the following protocol has been optimized for human lymphoblastoid cells. Minor variations (i.e. cell number, centrifugation speeds, and lysis conditions) may be required to optimize for your particular application. We have seen that crosslinking greatly reduces library efficiency, and therefore we recommend starting with fresh unfixed cells.
What you’ll need
- 2x TD Buffer (recipe below)
- lysis buffer (10 mM Tris-HCl, pH7.4, 10 mM NaCl, 3 mM MgCl, 0.1% IGEPAL CA-630)
- Tn5 Transposase (Illumina Cat #FC-121-1030)
- Qiagen PCR Cleanup Kit
- 10,000x SYBR Green I (Invitrogen Cat #S-7563)
- NEBNext High-Fidelity 2x PCR Master Mix (New England Labs Cat #M0541)
- 1.5mL DNA LoBind tubes (to be used for all steps in this protocol
- Harvest your cells (no fixation). How exactly you do this will depend on your particular tissue, cell type of interest, and experimental system.
- Spin down 50,000 cells at 750 ×g for 5 min, 4°C.
- Very slowly remove the liquid. Wash once with 50 μL of cold 1x PBS buffer. DO NOT PIPET UP AND DOWN.
- Spin down at 750 ×g for 5 min, 4°C.
- Very slowly remove the liquid. Gently pipette to resuspend (just 3 times up and down) the cell pellet in 50 μL of cold lysis buffer.
- Incubate on ice for 2 minutes.
- Spin down immediately at 750 ×g for 10 min, 4°C.
- Discard the supernatant, and immediately continue to transposition reaction.
Transposition Reaction and Purification
- Make sure your cell pellet is on ice, and make the following transposition reaction mix
2x TD Buffer
50 uL total
- Gently pipette to resuspend nuclei in the transposition reaction mix. Pipet up and down 10 times.
- Incubate the transposition reaction at 37°C for 45 min (mouse) or 30 min (human).
- Immediately following transposition, purify using a Qiagen MinElute Kit. Follow kit instructions —check pH!
- Elute transposed DNA in 10 μL Elution Buffer (10mM Tris buffer, pH 8). Allow EB buffer to incubate for 5min on column, then spin.
- To amplify transposed DNA fragments, combine the following:
Illumina Primer 1
Illumina Primer 2
100x SYBR Green I
10,000x SYBR Green I is diluted in EB Buffer to make a 100x working solution.
NEBNext High-Fidelity 2x PCR Master Mix
5o uL total
Purification of Final RNA-Seq Library Using AMPure Beads
Quality Check of Final Product
Normalize and Pool
- If not done already, quantify each of your libraries on Qubit. For most libraries, using the HS dsDNA Qubit assay with 2uL of input will yield a reading. Record the concentration in ng/uL for each library.
- Run your samples on Tapestation with either the D1000 or the HSD1000 assay. Remember to allow Tapestation reagents to sit at room temperature for at least 30 minutes before use. Save your Tapestation results by going to File -> Create Report -> Save as pdf. This file can then be emailed or uploaded to Asana. For the base pair length, we usually use the value of the peak identified by the Tapestation analysis software. This value is shown both on the tracing itself and in the Peak Table for each sample.
- Download our nM Conversion Calculator here. Enter the concentration (from Qubit) and the base pair length (from Tapestation) in the appropriate cells and it will give you the nM concentration for each library. Normalize and pool all your libraries to 4, 2, 1, or 0.5 nM in a LoBind microcentrifuge tube. If you need to dilute your libraries, we recommend using at least 2uL to minimize pipetting errors. The example sheet of the calculator provides further detail.
- Quantify your pool on Qubit and enter into the calculator sheet to check that your pool is close to the nM concentration you normalized to.
Setup Run in Basespace
- Sign into Basespace, then go to the Prep tab, Biological Samples, and select Import Samples on the upper right. Use Illumina’s Sample Import Template to enter information about your samples. The SampleID and Name can be the same, but make sure they are unique for each sample. Species can be left blank. Upload the completed .csv to import your samples.
- Continue to Prep Libraries. Select the library prep kit “TruSeqHT” If you used another index format, you will need to use a different entry for library prep kit. The your project name as the Plate ID. For each sample, check the box next to it on the left, then drag the sample name to the appropriate index well.
- Proceed to Pool Libraries. Select all your samples on the left, then drag and drop in the pool on the right. Name the pool your project name.
- Continue to Plan Run. Select NextSeq and name your run your project name. Select Single Read or Paired End Read, then enter the cycle numbers based on your selected kit. For example, if you were doing a run using a High Output 75 Cycle kit, you would select Single Read and enter 76 for Read 1 Cycles and 0 for Read 2 Cycles.
- Press Sequence to complete planning the run. The run will now be available for selection on the sequencer.
Loading the Sequencer
- The next step is to dilute and denature the prepared libraries. Illumina’s general guidelines for this on the NextSeq can be found here.
- Illumina’s system guide for the NextSeq, which covers the sequencing workflow, can be found here.
- Your final loading concentration should be 1.3 - 1.8 pM, with most pools loaded at 1.4 or 1.5 pM.