DNasing RNA, Round I

According to the QuantSeq library prep protocol, I need to ensure no DNA contamination in my RNA samples. Sam advises that all RNAzol-processed samples will definitely have some DNA contamination. So, I am using the Turbo DNase kit to clean my RNA.

July 31st - DNased RNA, qPCR to identify DNA contamination, batch 1 (n=30)

I ran a first batch of reactions (n=30) using the Turbo DNase kit. The kits we had in the -20 freezer were old (from 2014), so I walked over to the BioSciences stock room (J wing) and purchased 2 new kits (50 reactions per; I’ll need a couple more kits). NOTE: each kit is ~$145.

Turbo DNA Protocol

All reactions used 50 uL RNA, as per the manual’s example. Here were my steps:

  • Labeled 2 sets of 0.5 mL microcentrifuge tubes with RNA sample names
  • Transfered 1 uL of DNase into one set of tubes
  • Transfered 5 uL of Turbo DNase Buffer into each tube
  • Transfered 50 uL of RNA into tubes
  • Mixed gently - used low setting on the vortexer.
  • Incubated at 37C - used the thermocycler in FTR 209 - for 20 minutes
  • Removed samples from thermocycler, added 5 uL inactivation reagent solution. Prior to pipetting this inactivation reagent, I vortexted it thoroughly.
  • Incubated at room temperature for 5 minutes. Vortexed each sample briefly twice during this incubation time to keep solution mixed.
  • Centrifuged samples for 90 seconds at 10,000 rcf
  • Carefully transferred supernatant to fresh, labeled tubes.
  • Held DNased RNA on ice, while I learned how to run qPCR

qPCR to assess DNA contamination

I will use the SsoFast enzyme, a DNA polymerase technology that performs a super fast reaction, and the BIORAD CFX Connect qPCR machine.

Protocol:

  1. Created mastermix for PCR reactions for a total of 64 wells. The following table shows volumes needed for 1 pCCR reaction, then volumes needed for a mastermix for 64 reactions:
  per reaction 7/31/19
# Samples 1 30
# Reactions 1.0 62
Template (RNA sample) (uL) 1.0 62.0
Sso Fast (uL) 10.0 682.0
Pf, 10 uM (uL) 0.5 34.1
Pr, 10 uM (uL) 0.5 34.1
DEPC-treated water (uL) 8.0 545.6
Total Volume in mastermix (uL) 20.0 1,357.8

Following Sam’s lab notebook entry, I used elongation factor primers to check for DNA contamination:

  • EF1_qPCR_5’ (SRID 309) (Forward primer, Pf, SRID = 310)
  • EF1_qPCR_3’ (SRID 310) (Reverse primer, Pr, SRID = 309)

These primer stocks are stored in a small fridge in FTR 213, and can be found using the primer database. The stock concentrations are 100 micromolar. I need to use a working stock at 10 uM, so I melted the stocks and diluted 15 uL of each stock in 135 uL DEPC-treated ultrapure water (150 uL total volume).

The total volume per reaction is 20 uL. After creating the mastermix, I pipetted 19 uL of mastermix into a qPCR well plate. NOTE: the type of plate is specific - it’s a white plate, and “low profile” - which is specified on the qPCR software. I then pipetted 1 uL of each sample (i.e. template), in duplicate, to the well plate. I loaded samples horizontally (A1, A2, A3 … etc.) for ease of reading data downstream. In addition to including a control sample, which has been processed alongside the other samples since homogenization (sample 571), I included a No Template Control (NTC, 1uL water added instead of a sample), and DNA isolated from Oly larvae back in March 2018 (sample 69a, RNA sample 8a) as a positive control. To seal the plate I used the clear tape-like cover, rather than the clear plastic caps. I did not vortex the well plate prior to the qPCR reaction.

I carried the well plate over to the qPCR room, loaded it onto the CFX Connect, and opened the MAESTRO software on the adjacent computer. I used the Wizard to help configure the run. Here are the steps to execute the run:

Select “User Defined”

Capture01

Select Protocol: “CFX_2StepAmp_EVAGreen+Melt.prcl”

Capture02

Select plate file: “QuickPlate_96 wells_sybr_white.pltd” - this ensures that all wells are measured. We don’t assign sample names prior to running, but can edit the data file after completion.

Capture03

Select “Next”

Capture04

Select “Save” - it will automatically save the file to Owl and filename will include the run date.

Capture05

This is a screenshot immediately upon protocol initiation

Capture06

I downloaded MAESTRO to my computer (Mac version), and edited the plate setup to include sample names, and color coded melt curves by sample type: GREEN is positive control (n=2); RED is NTC (n=1), and PINK is the homogenization/isolation/DNase control (n=1); BLUE are the samples.

image

Data and report are saved on github in the O.lurida_Stress repo.

The melt curve doesn’t look like Sam’s recent run. However, I realize that the primers were not O. lurida, but were C. gigas. I didn’t think to ask whether the primers needed to be O. lurida specific, but I’m guessing yes. I will plan to move forward with the next batch of Turbo DNase-ing, and will figure out which primers are optimal. Interestingly I did see some DNA, and a melt temperature, for the positive controls, but the fluorescence was not as high as Sam’s example. Also interesting is that my homogenization/isolation control (pink) had a weird peak, suggesting some contamination.

image

Here ares ome qPCR notes from Sam’s instructions:

  • Keep RNA on ice while working with them, and store in -80 always.
  • There are 2x SsoFast aliquots in the fridge, and also in the freezer in the “PCR supplies” box in the -20 (both in FTR 209).
  • Mastermixes should be used the same day they are prepared, but can sit on ice for a few hours.
  • qPCR plates can be prepared, then sealed and held in the fridge for a bit. For example, I could prepare one qPCR plate, then while it is running I can prepare another and hold it in the fridge until the machine is ready again.
  • Always use the button to open/close the BioRAD CFX Connect lid - don’t manually close the lid

Quantified DNased RNA

Used Qubit HS RNA to measure RNA concentration in DNased samples. Approximate volume remaining for DNased RNA is 50 uL. I find it odd that some of my samples have more concentrated RNA after the DNasing. I will look in to that.

Date larvae collected Cohort Treatment TISSUE SAMPLE # Homo./RNA TUBE # VOL RNAzol (mL) MASS TISSUE (mg) [RNA] ng/uL Volume for DNase treatment Amount of RNA in Dnase treatment (ug), max is 10 ug Date Turbo Dnase treatment [RNA] after Turbo Dnase treatment
5/24/17 Dabob Bay 10 Ambient 14-A 401 1 100 52.0 50 2.60 7/31/19 93.4
5/31/17 Dabob Bay 10 Ambient 31-A 402 1 10 140.0 50 7.00 7/31/19 114.0
5/26/17 Dabob Bay 10 Low 23-A 411 1 10 57.2 50 2.86 7/31/19 72.6
5/27/17 Dabob Bay 10 Low 27-A 412 1 10 60.8 50 3.04 7/31/19 31.2
6/12/17 Dabob Bay 6 Ambient 59-A 421 1 10 43.0 50 2.15 7/31/19 57.6
6/7/17 Dabob Bay 6 Low 51-A 431b 1 20 61.2 50 3.06 7/31/19 83.0
6/17/17 Dabob Bay 6 Low 72-A 432 1 50 47.6 50 2.38 7/31/19 74.0
5/25/17 Fidalgo Bay 10 Ambient 20-A 441 1 70 46.0 50 2.30 7/31/19 16.2
6/3/17 Fidalgo Bay 10 Ambient 38-A 442b 1 80 56.2 50 2.81 7/31/19 69.8
5/24/17 Fidalgo Bay 10 Low 16-A 451 1 70 68.4 50 3.42 7/31/19 68.4
5/24/17 Fidalgo Bay 10 Low 18-A 452b 1 80 48.4 50 2.42 7/31/19 97.2
5/26/17 Fidalgo Bay 6 Ambient 22-A 461b 1 100 54.0 50 2.70 7/31/19 84.0
5/29/17 Fidalgo Bay 6 Ambient 29-A 462b 1 60 69.8 50 3.49 7/31/19 106.0
5/25/17 Fidalgo Bay 6 Low 19-A 471b 1 100 71.0 50 3.55 7/31/19 108.0
5/26/17 Fidalgo Bay 6 Low 21-A 472b 1 70 64.0 50 3.20 7/31/19 97.0
5/20/17 Oyster Bay C1 10 Ambient 02-A 481 1 40 64.4 50 3.22 7/31/19 89.2
5/20/17 Oyster Bay C1 10 Ambient 04-A 482 1 60 67.2 50 3.36 7/31/19 22.2
5/23/17 Oyster Bay C1 10 Ambient 09-A 484 1 40 66.2 50 3.31 7/31/19 58.4
6/15/17 Oyster Bay C1 10 Ambient 66-A 491 1 20 126.0 50 6.30 7/31/19 58.4
6/14/17 Oyster Bay C1 10 Low 62-A 506 1 80 63.8 50 3.19 7/31/19 29.2
6/5/17 Oyster Bay C1 6 Ambient 45-A 513   30 156.0 50 7.80 7/31/19 142.0
5/21/17 Oyster Bay C1 6 Low 01-A 521 1 70 54.4 50 2.72 7/31/19 66.6
5/22/17 Oyster Bay C1 6 Low 07-A 522 1 20 60.8 50 3.04 7/31/19 32.2
6/15/17 Oyster Bay C1 6 Low 68-A 528 1 30 162.0 50 8.10 7/31/19 87.6
5/24/17 Oyster Bay C2 10 Ambient 17-A 531 1 60 88.2 50 4.41 7/31/19 95.4
5/23/17 Oyster Bay C2 10 Low 12-A 541 1 40 45.6 50 2.28 7/31/19 44.4
5/24/17 Oyster Bay C2 10 Low 13-A 542 1 30 82.0 50 4.10 7/31/19 32.8
6/3/17 Oyster Bay C2 6 Ambient 41-A 552b 1 80 64.8 50 3.24 7/31/19 74.6
5/21/17 Oyster Bay C2 6 Low 05-A 561 1 40 43.4 50 2.17 7/31/19 28.0
NA RNA Control RNA Control   571 1 10 LOW 50 LOW 7/31/19 LOW
Written on July 31, 2019