Using a Fluorescent PCR-capillary Gel Electrophoresis Technique to Genotype CRISPR/Cas9-mediated Knockout Mutants in a High-throughput Format

Summary

The genotyping technique described here, which couples fluorescent polymerase chain reaction (PCR) to capillary gel electrophoresis, allows for high-throughput genotyping of nuclease-mediated knockout clones. It circumvents limitations faced by other genotyping techniques and is more cost effective than sequencing methods.

Abstract

The development of programmable genome-editing tools has facilitated the use of reverse genetics to understand the roles specific genomic sequences play in the functioning of cells and whole organisms. This cause has been tremendously aided by the recent introduction of the CRISPR/Cas9 system-a versatile tool that allows researchers to manipulate the genome and transcriptome in order to, among other things, knock out, knock down, or knock in genes in a targeted manner. For the purpose of knocking out a gene, CRISPR/Cas9-mediated double-strand breaks recruit the non-homologous end-joining DNA repair pathway to introduce the frameshift-causing insertion or deletion of nucleotides at the break site. However, an individual guide RNA may cause undesirable off-target effects, and to rule these out, the use of multiple guide RNAs is necessary. This multiplicity of targets also means that a high-volume screening of clones is required, which in turn begs the use of an efficient high-throughput technique to genotype the knockout clones. Current genotyping techniques either suffer from inherent limitations or incur high cost, hence rendering them unsuitable for high-throughput purposes. Here, we detail the protocol for using fluorescent PCR, which uses genomic DNA from crude cell lysate as a template, and then resolving the PCR fragments via capillary gel electrophoresis. This technique is accurate enough to differentiate one base-pair difference between fragments and hence is adequate in indicating the presence or absence of a frameshift in the coding sequence of the targeted gene. This precise knowledge effectively precludes the need for a confirmatory sequencing step and allows users to save time and cost in the process. Moreover, this technique has proven to be versatile in genotyping various mammalian cells of various tissue origins targeted by guide RNAs against numerous genes, as shown here and elsewhere.

Introduction

Reverse genetic approaches have allowed scientists to elucidate the effects of specific alterations in the genome on the cell or whole organism. For example, the expression of a particular gene can be attenuated by gene knockdown^1,2 (partial reduction) or gene knockout^3,4 (complete ablation) in order to determine the effect that this has on the function of the cell or on the development of the organism.

Gene knockout experiments have become easier since the introduction of sequence-specific programmable nucleases, such as zinc-finger nucleases (ZFNs) and transcription activator-like effector nucleases (TALENs). However, the relatively recent characterization of the clustered regularly interspersed short palindromic repeat (CRISPR)/Cas9 system has made it extremely easy for any laboratory around the world to perform gene knockout experiments. In essence, the CRISPR/Cas9 system consists of two essential components-a single guide RNA (sgRNA), which recognizes and binds via base complementarity to a specific sequence in the genome, and an endonuclease called Cas9. The aftermath of the specific binding and action of the sgRNA-Cas9 complex on genomic DNA is the double-strand cleavage of DNA. This, in turn, triggers the DNA damage response mechanism in the cell, which is subsequently repaired via the non-homologous end-joining (NHEJ) or homologous recombination (HR) pathways. Since the NHEJ repair mechanism (but not the HR mechanism) often results in the random insertion or deletion of nucleotides at the site of repair, resulting in insertion/deletion (indel) mutations, it may cause the reading frame of an exon to shift. This may then result in the knockout of the gene due to premature termination of translation and nonsense-mediated decay^5,6,7.

Despite the convenience afforded by the introduction of the CRISPR/Cas9 system in knocking out a gene, the genotyping of clones of targeted cells remains a bottleneck, especially in a high-throughput setting^8,9. Existing techniques either suffer major inherent limitations or are financially costly. For example, the SURVEYOR or T7E1 assay, which is an enzymatic assay that detects mismatches in DNA duplexes¹⁰, is not able to distinguish between wildtype clones and homozygous mutants (clones whose alleles are mutated identically), since these clones have identical alleles and thus do not present mismatches in their DNA sequence¹¹. In addition, the use of Sanger sequencing, which is considered the gold standard in genotyping mutant clones, in a high-throughput setup is undesirable due to its high cost. Here, we present a detailed protocol of the fluorescent PCR-capillary gel electrophoresis technique, which can circumvent the limitations of the other existing genotyping techniques and is particularly useful in performing a high-throughput screen of nuclease-mediated knockout clones. This method is technically simple to perform and saves time and cost.

Protocol

1. Obtaining CRISPR/Cas9-targeted Single-cell Clones

1. Seed HEPG2 cells on a 6-well plate at 500,000 cells per well in 2 mL of antibiotic-free Dulbecco's Modified Eagle Medium (DMEM) supplemented with 10% fetal bovine serum (FBS). Incubate for 24 h at 37 °C and 5% CO₂.
2. Transfect cells with plasmid co-expressing Cas9 and specific sgRNA against the gene of interest using an appropriate transfection reagent as per the manufacturer's instructions.
   NOTE: For example, sgRNA can be cloned into the pSpCas9(BB)-2A-GFP vector, as described previously⁴.
3. Replace the culture medium 4 - 16 h after transfection with 2 mL of fresh antibiotic-free medium.
4. About 48 h after transfection, collect single-cell suspension by trypsinizing the cells.
   1. Trypsinize the cells in 0.2 mL of 0.25% trypsin-EDTA and incubate at 37 °C for 5 min. Add 1 mL of medium and resuspend thoroughly.
5. Sort the cells for GFP-positive clones, as described previously¹², and collect about 3,500 cells.
6. Plate the GFP-positive sorted cells on 10-cm dishes at 500, 1,000 and 2,000 cells per dish in 8 mL of penicillin/streptomycin-supplemented culture medium. Incubate the cells at 37 °C and 5% CO₂.
7. Maintain the cells at 37 °C and 5% CO₂, replacing the medium every five days, until they grow into single-cell colonies large enough to be visible to the naked eye. For most cancer cell lines, this takes about two weeks from day of plating.
8. When the colonies are of the appropriate size (i.e., visible to the naked eye), transfer individual colonies to wells of a 96-well culture plate containing 200 µL of DMEM supplemented with 10% FBS.
   1. Aspirate the single-cell colonies using a 200-µL pipette with a small volume of medium. Resuspend the cells thoroughly in individual wells by triturating several times.
9. Maintain the cells at 37 °C and 5% CO₂, replacing the medium every five days, until they reach 50 - 90% confluence. For most cancer cell lines, this takes about 24 - 48 h.

2. Extracting Crude Genomic DNA Using a Direct Lysis Method

1. When the cells reach 50 - 90% confluence, remove as much of the culture medium from the wells as possible using multi-channel vacuum suction or a multi-channel pipette.
2. Add 25 µL of 0.05% trypsin-EDTA (without phenol red) into each well and incubate at 37 °C for 7 min.
3. Resuspend the trypsinized cells thoroughly by pipetting up and down several times. Check the cells under a microscope to make sure that they are detached from the plastic surface.
4. Create a replicate of the individual clones by transferring approximately 5 µL of the single-cell suspension to an empty 96-well culture plate. Add 200 µL of culture medium to each well and maintain the cells until positive clones are identified using fluorescent PCR-capillary gel electrophoresis (see below). Serially expand the cells to 10-cm dishes or any other scale of choice (see section 7).
5. Add 5 µL of the single-cell suspension from step 2.3 to 10 µL of homemade direct-lyse buffer (10 mM Tris pH 8.0, 2.5 mM EDTA, 0.2 M NaCl, 0.15% SDS, and 0.3% Tween-20)¹² in a 96-well PCR plate and mix thoroughly by pipetting up and down several times. Centrifuge briefly (to bring the liquid down to the bottom of the wells).
6. Add 200 µL of culture medium to the remaining ~ 15 µL of cell suspension from step 2.3 and incubate at 37 °C and 5% CO₂, together with the replicate from step 2.4.
7. Subject the lysates from step 2.5 to the following thermal cycling program to ensure complete lysis of the cells and release of genomic DNA: 65 °C for 30 s, 8 °C for 30 s, 65 °C for 1.5 min, 97 °C for 3 min, 8 °C for 1 min, 65 °C for 3 min, 97 °C for 1 min, 65 °C for 1 min, and 80 °C for 10 min. Centrifuge the lysates briefly.
8. Dilute the lysates by adding 40 µL of nuclease-free water and mix thoroughly using a vortex mixer. Centrifuge briefly. The diluted lysates can be used immediately or stored at -20 °C for several months without significant loss of quality.

3. Performing Fluorescent PCR to Amplify CRISPR/Cas9 Target Regions

1. Design two fluorophore-labeled forward primers (both labeled at the 5' end) for each CRISPR/Cas9 target region; cutting sites that are further than 300 bp from each other should be considered as two separate target regions (e.g., green fluorophore-labeled primer for untargeted wildtype control and blue fluorophore-labeled primer for CRISPR/Cas9-targeted clones; see the Table of Materials).
   1. Procure these labeled forward primers and an unlabeled reverse primer accordingly. Note that primers can be designed using any tool of choice and that the amplicons should be 200 - 500 bp long.
2. Perform PCR as described previously¹² to amplify target regions using the labeled primers.
   1. Use 3 µL of the diluted lysates from step 2.8 in a 20-µL reaction (see Table 1) and the following thermal cycling program: 94 °C for 10 min (1 cycle); 94 °C for 10 s, 64 °C for 30 s, 68 °C for 1 min (4 cycles); 94 °C for 10 s, 61 °C for 30 s, 68 °C for 1 min (4 cycles); 94 °C for 10 s, 58 °C for 30 s, 68 °C for 1 min (4 cycles); 94 °C for 10 s, 55 °C for 30 s, and 68 °C for 1 min (35 cycles).
3. Resolve 5 µL of the PCR amplicons on a 1% agarose gel to check for size and relative amount of amplicons¹².
   NOTE: Performing this step for all the samples is encouraged but not necessary; resolving a selected number of samples is sufficient to estimate the amount of amplicons present in the samples in general.

4. Preparing Samples for Capillary Gel Electrophoresis

1. Dilute amplicons of wildtype (untargeted parental cells) and CRISPR/Cas9-targeted DNA in nuclease-free water to approximately 2.5 ng/µL. Make sure to dilute enough wildtype DNA sample to be added to each targeted DNA sample (a minimum of 0.5 µL of diluted wildtype sample per targeted sample is required).
2. Mix the diluted wildtype and targeted DNA samples in equal ratio (e.g., mix 1 µL of wildtype sample with 1 µL of targeted sample).
3. Add 1 µL of the mixed amplicons to 8.7 µL of deionized formamide and 0.3 µL of dye-labeled size standard in a 96-well PCR plate that is compatible with the genetic analyzer.
   NOTE: The use of a master mix of the formamide and the size standard (i.e., a preparation of a premix of the formamide and the size standard in a 29:1 ratio prior to the addition of amplicons to ensure standardized amounts) is recommended.
4. Tightly seal the plate and heat the samples at 95 °C for 3 min using a PCR thermocycler.
5. Place the plate on ice immediately after the heating step and incubate for at least 3 min.

5. Performing Capillary Gel Electrophoresis on a Genetic Analyzer

1. Set up assay parameters, instrument protocol, and size-calling protocol on the capillary gel electrophoresis software connected to a genetic analyzer.
   NOTE: This step is only required for the first electrophoresis run; the program can be saved for future use. For subsequent runs, go straight to step 5.2.
   1. Click on the "Create New Plate" icon on the software dashboard.
   2. Give the run a dummy name and select the following options: Number of wells, 96; Plate Type, Fragment; Capillary Length, 50 cm; and Polymer, POP7. Click on the "Assign Plate Content" button.
   3. Under "Assays," click "Create New Assay"; a new panel will appear.
   4. Name the assay "FPCR-CGE Assay" and check that "Application Type" is correctly set as "Fragment."
   5. Set up instrument protocol by clicking on the "Create New" button under "Instrument Protocol."
      1. Set or choose the following options and parameters in the appropriate areas: Application Type, Fragment; Capillary Length, 50 cm; Polymer, POP7; Dye Set, G5; Run Module, FragmentAnalysis; Protocol Name, FPCR-CGE Instrument Protocol; Oven Temperature, 60 °C; Run Voltage, 19.5 kV; Pre-run Voltage, 15 kV; Injection Voltage, 1.6 kV; Run Time, 1,330 s; Pre-run Time, 180 s; Injection Time, 15 s; and Data Delay, 1 s.
   6. Click on the "Apply to Assay" button and then the "Save to Library" button to save the program. Close the panel to continue.
   7. Set up a size-calling protocol by clicking on the "Create New" button under "Sizecalling Protocol."
      1. Set or choose the following options and parameters in the appropriate areas: Protocol Name, FPCR-CGE Sizecalling Protocol; Size standard, GS500(-250)LIZ; Size-caller, SizeCaller v1.1.0; Analysis Settings,-; Analysis Range, Full; Sizing Range, Full; Size Calling Method, Local Southern; Primer Peak, Present; Blue, Green, Orange Channels, (Check); Minimum Peak Height, 175 for all channels; Use Smoothing, None; Use Baselining (Baseline Window (Pts)), (Check) 51; Minimum Peak Half Width, 2; Peak Window Size, 15; Polynomial Degree, 3; Slope Threshold Peak Start, 0.0; Slope Threshold Peak End, 0.0; QC Settings, -; Size Quality, -; Fail if Value is <0.25; Pass if Value is <0.75; Assume Linearity from 0 bp to 800 bp; and Actuate Pull-Up flag if Pull-Up Ratio ≤ 0.1 and Pull-Up Scan ≤ 1.
   8. Click on the "Apply to Assay" button and then the "Save to Library" button to save the program. Close the panel to continue.
   9. Ensure that the assay is saved by clicking on the "Save to Library" button once more and exit the panel by clicking the "Close" button.
   10. Back at the "Assign Plate Contents" page, click on the "Create New File Name Convention" link under "File Name Conventions."
   11. Name the program "FPCR-CGE File Name."
   12. Under "Available Attributes," select the desired attributes that will appear in the file name (such as "Date of Run," "Time of Run," "Well Position," and "Sample Name"). Choose the desired file location where the results of the run will be stored.
   13. Click on the "Apply to Assay" button and then the "Save to Library" button to save the program. Close the panel to continue.
   14. Back at the "Assign Plate Contents" page, click on the "Create New Results Group" link under "Results Groups."
   15. Name the program "FPCR-CGE Results Groups."
   16. Under "Available Attributes," select the desired attributes that will appear in the file name (such as "Assay Name"). Choose the desired file location where the results of the run will be stored.
   17. Click on the "Apply to Assay" button and then the "Save to Library" button to save the program. Close the panel to continue.
2. Set up the program for an electrophoresis run by following the steps below.
   1. Go to the dashboard and click on the "Create New Plate" icon.
   2. Name the run as desired (for easy reference, include the date, cell line, and gene name). Select the following options: Number of wells, 96; Plate Type, Fragment; Capillary Length, 50 cm; and Polymer, POP7. Click on the "Assign Plate Content" button.
   3. Label each well of the sample as desired (e.g., a sample can be named "NC" to indicate that the well is a negative control).
   4. Under the "Assays," "File Name Conventions," and "Results Groups" boxes, click the "Add from Library" link and select the programs created in step 5.1.3 to 5.1.17.
   5. Highlight all the wells to be analyzed and select the relevant programs under "Assays," "File Name Conventions," and "Results Groups" by checking the boxes next to them.
3. Before loading the plate on the tray of the genetic analyzer, apply the rubber seal on the 96-well plate and put the sealed plate in the plastic case that comes with the genetic analyzer.
4. Push the "Tray" button at the front of the genetic analyzer, and when the tray reaches the front of the equipment, open the door and load the encased plate on the tray. Ensure that the plate is locked in place and then close the door.
5. Click on the "Link Plate for Run" button.
6. In the "Load Plates for Run" page, do a final check to ensure that all the reagents and conditions are correct and in order.
7. Click on the "Start Run" button. Each run of 24 samples (the first 3x8 wells of the 96-well plate) takes less than 55 min to complete.

6. Analysis of the Electropherogram to Determine Base-pair Differences

1. When the capillary gel electrophoresis run is complete, open the analysis software to analyze the results.
2. Click on the "Add Samples to Project" icon and search for the folder containing the run files. Recall from step 5.1.12 the assigned location of the results files.
3. Select all the results files of each injection in the completed run and click on the "Add to List" button; the names of these files begin with "Inj" and contain the details of the run.
4. Click the "Add and Analyze" button to proceed with the analysis.
5. Select all the samples in the run by clicking on the first sample and dragging the cursor down to the last sample and then click the "Display Plots" icon.
6. To check the quality of the size standard, open the orange channel of the results by checking the orange icon and unchecking the rest of the colored icons; this is important to ensure that the size-calling is accurate and reliable.
7. To view the peaks corresponding to the fragments derived from the untargeted control and the targeted clones, check the blue and green icons to open readings from these channels.
8. Place the cursor over the horizontal axis of the first results plot and right-click to select "Full View." Scroll down to view all the results at a glance to determine if there is any major problem with the run. To zoom in on a specific range of values, right-click the mouse on the relevant axis of the plot, choose "Zoom To…," and key in the range of values of interest.
   NOTE: One potential major problem is that all the samples give low intensity peaks. This is usually due to the prolonged storage of fluorophore-labeled amplicons prior to the capillary electrophoresis run or the over-dilution of amplicons, which can easily be rectified by repeating the PCR step or by diluting the amplicons using a lower dilution factor, respectively.
9. To save the results, follow the steps described below.
   1. Ensure that the blue and green channels are selected and click on the "Sizing Table" icon.
   2. Save the table of values in tab-delimited text (.txt) format by opening "File" and choosing "Export Table." Name the file accordingly and select the file location of choice.
   3. To save the plots of the run in PDF format, go to "File" and click on the "Print" option. Choose the relevant PDF writer and press "Print." Name the file accordingly and select the file location of choice.
10. To calculate the difference in the size of the fragments derived from untargeted wildtype control and the CRISPR/Cas9-targeted clones, follow the steps described below.
    1. Open the tab delimited text (.txt) file from step 6.9.2 with a spreadsheet program. The table should include these four important columns: "Dye/Sample Peak" (indicating a blue or green channel), "Sample File Name" (the first characters indicate the well or sample name), "Size" (indicating the size of the fragment called), and "Height" (indicating the fluorescence intensity of the peak).
    2. To single out relevant peaks, exclude those that are not in the expected size range.
       NOTE: Typically, indel mutations rarely result in more than a 100-bp difference in size; thus, peaks whose size differs by more than 100 bp from the wildtype control peak (dominant peak in the green channel) are excluded. This can be easily done by using the "Between" option under the "Conditional Formatting" function in the spreadsheet.
    3. To remove non-specific peaks, which are indistinguishable from background level, use the "Less Than" option under the "Conditional Formatting" function in the spreadsheet program to exclude peaks whose heights are lower than 2,000 units. This cut-off value has been empirically determined and can therefore be adjusted where deemed fit.
    4. Calculate the difference in fragment size between each of the resulting peaks in the blue channel (CRISPR/Cas9-targeted clones) and the sole peak in the green channel (untargeted wildtype control) by subtracting the latter from the former.
       NOTE: It is important to use values attributed to each capillary electrophoresis sample, as there may be inter-sample differences in the fragment size of the wildtype control.
    5. Round off the values to the nearest integer to determine the number of base pairs that have been inserted into or deleted from, if any, the genomic sequence in question. When knocking out a gene is of interest, select clones whose indel mutations are not of multiples of 3 bp to ensure that there is frameshift in the coding sequence.

7. Verification of the Knockout Status of Clones

1. Expand individual knockout clones from the 96-well plate (from steps 2.4 and 2.6) to a 24-well plate by trypsinizing the cells using 25 µL of 0.25% trypsin-EDTA and incubating at 37 °C for 5 min.
2. Add 125 µL of medium (DMEM supplemented with 10% FBS) to the trypsinized cells and resuspend thoroughly.
3. Transfer the cell suspension to a 15-mL tube and centrifuge at 400 x g for 5 min at room temperature.
4. Remove as much of the medium as possible using vacuum suction or a pipette, resuspend the cell pellet in 500 µL of medium, and transfer the cell suspension to a well of a 24-well plate. Incubate at 37 °C and 5% CO₂ until the cells reach 80-90% confluence.
5. Expand the individual clones serially from the 24-well plate to a 6-well plate and from the 6-well plate to a 10-cm dish when they reach 80 - 90% confluence by repeating steps 7.1 to 7.4, using the following volumes: 50 µL of 0.25% trypsin-EDTA and 150 µL of medium (for expanding from the 24-well plate to the 6-well plate) and 200 µL of 0.25% trypsin-EDTA and 1 mL of medium (for expanding from the 6-well plate to the 10-cm dish).
6. Harvest the clones when they reach 80 - 90% confluence by trypsinizing the cells using 1 mL of 0.25% trypsin-EDTA and incubate at 37 °C for 5 min.
7. Add 5 mL of medium (DMEM supplemented with 10% FBS) to the trypsinized cells and resuspend thoroughly.
8. Transfer the cell suspension equally into two 15-mL tubes, centrifuge at 400 x g for 5 min at room temperature, and remove the medium as much as possible. One portion of the cells is for genomic DNA extraction and the other is for total protein extraction.
9. For verification via Sanger sequencing, follow the steps described below.
   1. Extract genomic DNA from the clones as described previously¹².
   2. Perform PCR amplification of the region spanning the CRISPR/Cas9 target site, as described in section 3.2, but use unlabeled primers. Do not use labeled primers for this step, as the fluorescence from the tag will interfere with the subsequent Sanger sequencing step.
   3. Purify the amplicons using a PCR clean-up kit, as described previously¹².
   4. Sequence the purified amplicons using the PCR primers used in step 7.9.2 to determine the genotype of the clones, as described previously¹².
10. For verification via Western blot analysis, extract total protein from the wildtype cells and targeted clones, as described previously¹².
    1. Perform Western blot analysis using appropriate antibodies against the protein of the target gene, as described previously¹²; a true knockout clone is devoid of the expression of the protein.

Results

The fluorescent PCR-capillary gel electrophoresis technique described here is anticipated to be applicable to any targetable region in the genome in virtually any cell line that is amenable to foreign DNA delivery. We have previously demonstrated its application by targeting three genes in a colorectal cancer cell line¹². Here, we show its efficacy in genotyping a hepatocellular carcinoma cell line, HEPG2, targeted with a CRISPR/Cas9 construct against the Nucleosom...

Discussion

The knocking out of a specific gene in a model cell line of choice has become routine for elucidating the role that the gene plays in that particular cellular context. In fact, several genome-wide screens are currently available that use the CRISPR/Cas9 system to target virtually all known human genes in the genome^14,15,16. With these large-scale screens (or even small-scale targeting of individual genes of interest), it is impo...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
HEPG2 cells	ATCC	HB-8065
HyClone Dulbecco's Modified Eagles Medium (DMEM)	Thermo Fisher Scientific	SH30022.01
HyClone Fetal Bovine Serum	Thermo Fisher Scientific	SV30160.03
pSpCas9(BB)-2A-GFP plasmid	Addgene	PX458
Lipofectamine 2000	Thermo Fisher Scientific	11668027
Trypsin-EDTA (0.25%), phenol red	Thermo Fisher Scientific	25200056
Trypsin-EDTA (0.5%), no phenol red	Thermo Fisher Scientific	15400054
Penicillin-Streptomycin (10,000 U/mL)	Thermo Fisher Scientific	15140122
HyClone Water, Molecular Biology Grade	GE Healthcare	SH30538.02
CRISPR sgRNA insert oligonucleotide (sense)	AITbiotech	None	Sequence: 5'-CACCGCTAACCTTTCAGCCTGCCTA-3'
CRISPR sgRNA insert oligonucleotide (anti-sense)	AITbiotech	None	Sequence: 5'-AAACTAGGCAGGCTGAAAGGTTAGC-3'
Unlabeled PCR amplification forward primer	AITbiotech	None	Sequence: 5'-CACTAACTCCAATGCTTCAGTTTC-3'; this primer is also used to sequence PCR amplified alleles
6-FAM-labeled fluorescent PCR forward primer	AITbiotech	None	Sequence: 5'-6-FAM-CACTAACTCCAATGCTTCAGTTTC-3'
HEX-labeled fluorescent PCR forward primer	AITbiotech	None	Sequence: 5'-HEX-CACTAACTCCAATGCTTCAGTTTC-3'
Unlabeled PCR reverse primer	AITbiotech	None	Sequence: 5'-CCTCTTCCAAGTCTGCTTATGT-3'
Taq PCR Core Kit	QIAGEN	201223
Hi-Di Formamide	Thermo Fisher Scientific	4311320
GeneScan 500 LIZ Dye Size Standard	Thermo Fisher Scientific	4322682
MicroAmp Optical 96-Well Reaction Plate	Thermo Fisher Scientific	4306737
3500xL Genetic Analyzer	Thermo Fisher Scientific	4405633
3500 Series 2 program	Thermo Fisher Scientific	4476988
Gene Mapper 5 program	Thermo Fisher Scientific	4475073
Gentra Puregene Cell Kit	QIAGEN	1045696
Wizard SV Gel and PCR Clean-Up System	Promega	A9282
NAP1L1 Antibody (N-term)	Abgent	AP1920b
Nuclear Matrix Protein p84 antibody [5E10]	GeneTex	GTX70220
Peroxidase AffiniPure Goat Anti-Rabbit IgG	Jackson ImmunoResearch	111-035-144
Peroxidase AffiniPure Sheep Anti-Mouse IgG	Jackson ImmunoResearch	515-035-003