Tag Archives: PCR

Tuesday 11/24/15

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Finished gel extraction of samples B3-C4 from 2bRAD Library 1 started on 11/23/15 following the protocol described in that post.

Did the PCR of the rest of Library 1 (B5-C12) with the new Taq. There is no H9, however (due to how I labelled on the spreadsheet).

First made more Lib 1 and Lib 2 primer stock:

  • 10 uL stock + 90 uL NFW = 10 uM

PCR master mix. Added 3.75 of each 1 uM barcode (HT and BC) to wells.
1x
65
10 mM (each) dNTPS
1.5
97.5
10 uM ILL-Lib1
1.5
97.5
10 uM ILL-Lib2
1.5
97.5
5X Q5 buffer
15
975
Q5 Taq polymerase
.75
48.75
20.25 + barcode = 27.75
648

 

11/21/15 and 11/22/15

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Saturday 11/21/15

Added 8 uL of nuclease free water to Libraries 2, 3, and 4. Put in 4degC.

Sunday 11/22/15

Set up a PCR of wells H1-B4 of Library 1 (did not have enough Taq to do any more so ordered more Q5 High-Fidelity Taq). As the 100 uL PCR reactions recommended in the Meyer 2bRAD protocol always overfill my gel wells, I rescaled the recipe to be 77.75 uL reactions (50 uL ligation product + 3.75uL each barcode + 20.25 uL master mix).

First, made new working stocks of primers:

  • Made 10 uM stock of Lib 1 and Lib 2
    • 5 uL stock + 45 uL NFW
  • Made 1 uM stock of BC11, BC12, HT2, HT3, HT4, HT5, HT6, HT7, HT8
    • 1 sock + 99 NFW
1x
32
10 mM (each) dNTPS
2: 1.5
48
10 uM ILL-Lib1
2: 1.5
48
10 uM ILL-Lib2
2: 1.5
48
5X Q5 buffer
20: 15
480
Q5 Taq polymerase
1: .75
24
20.25
648

Added 3.75 uL of each barcode (this took a lot of time. I marked on the datasheet as I went to make sure I added barcodes to each well.)

Made a large gel with 24 wells and a regular gel with 8 wells. The top part of the large well broke so was only able to run 22 of the 31 PCRs (H1-C3). I put the gel slices in 1.5mL tubes with 40 uL of NFW and left overnight in the fridge.

Gel of samples H1-C2 from 2bRAD Library 1.
Gel of samples B2-C3 from 2bRAD Library 1.

Did the AlfI digestion of libraries 2, 3, and 4.

1x
230x
10x buffer R
1.2 uL
276
150 uM SAM
.8
184
AlfI (2 U/uL)
.5
115
water
1.5
345
4
920

Thermocycler at 37degC for 2 hours and 65degC for 15 minutes. Put in fridge afterwards.

Wednesday 10/14/15

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DNA Extraction of Oly Broodstock

  • SS1_1
    SS1_2 (not tan)
    SS1_3
    SS1_4
    SS1_5
    SS1_6
    SS1_7
    SS1_8
    SS1_9
    SS1_10
    SS1_11
    SS1_12
    SS1_13
    SS1_14
    SS1_15
    SS1_16
    SS1_17
    SS1_18
    SS1_19
    SS1_20
    SS3_1
    SS3_2
    SS3_5
    SS3_6
  • Found 2 tubes labelled SS1_2. Marked the unextracted one with a tan sticker
  • Could not initially find SS3_3 or SS3_4 but found later and reorganized box
  • Left in 60degC water bath for 3 hours
  • Eluted 50 uL then 100 uL

Primers

  • Received the rest of the 2b-RAD primers and resuspended them to 100 uM.
    • BC11
    • BC12
    • HT3
    • HT4
    • HT5
    • HT6
    • HT7
    • HT8
  • Made new 1 uM aliquots of BC2-10 and HT1
    • 1 uL stock + 99 uL NFW
  • Made new 10 uM  aliquots of Lib 1 and Lib 2
    • 2.5 uL stock + 22.5 uL NFW

PCR for 2b-RAD MiSeq run

Used 10 samples from 9/28/15 digestion and ligation. Numbers in parentheses are so I know which tube from the ligation each sample is in.

  1. SS2_6 (5)
  2. SS2_7 (6)
  3. SS2_8 (7)
  4. HC1_5 (8)
  5. HC1_6 (9)
  6. HC1_7 (10)
  7. HC1_8 (11)
  8. NF1_4 (14)
  9. NF1_5 (15)
  10. NF1_6 (16)

Master Mix
1x
10.5x
NFW
23 uL
241.5
10 mM (each) dNTPS
2
21
10 uM ILL-Lib1
2
21
10 uM ILL-Lib2
2
21
5X Q5 buffer
20
210
Q5 Taq polymerase
1
10.5
Added 50 uL of MM to 40 uL of ligation product. Added 5 uL of 1uM BC and HT to each sample, using BC1-10 and HT1.
Run out gel of 2b-RAD PCR product
This time, set up a medium gel for 8 of the samples and a small gel for the other 2. Made a 2% TAE gel, and after running it at 110V for 1 hour let the gels soak in water with 6 uL of EtBr to increase staining. PCR used 19 cycles.

Gel of 2b-RAD PCR product

Gel of 2b-RAD PCR product

20151015_124156

I think I should make sure to mix in the EtBr when doing the post staining as that is likely why there are bright white sections on the gels. It was still much easier to see the bands though. Cut out the bands and left them in 1.5 mL tubes in 4degC for gel extraction on Friday.

Tuesday 9/22/15

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Lab Work

Set up a test PCR to determine the optimum # of cycles. You want to identify the minimum number of cycles required for a visible product at 166 bp. I chose 4 of the samples and tested them at 12, 17, 22, & 27 cycles as recommend in the protocol.

  • Made 100 uM stock of new ILL-Lib2 adaptor
  • Made 10 uM stocks of ILL-Lib1 and ILL-Lib2 primers
    • 1.5 stock + 13.5 uL NFW
  • Made 1 uM stocks of HT1 and BC1
    • 1uL stock + 99 NFW
1x
17x
NFW
4.6 uL
78.2
10 mM (each) dNTPS
.4
6.8
10 uM ILL-Lib1
.4
6.8
10 uM ILL-Lib2
.4
6.8
1 uM ILL-HT1
1
17
1 uM ILL-BC1
1
17
5X Q5 buffer
4
68
Q5 Taq polymerase
.2
3.4
Added 12 uL master mix to 8 uL ligation.
  1. SS2_3_12x
  2. HC1_1_12x
  3. NF1_1_12x
  4. NF1_2_12x
  5. SS2_3_17x
  6. HC1_1_17x
  7. NF1_1_17x
  8. NF1_2_17x
  9. SS2_3_22x
  10. HC1_1_22x
  11. NF1_1_22x
  12. NF1_2_22x
  13. SS2_3_27x
  14. HC1_1_27x
  15. NF1_1_27x
  16. NF1_2_27x

17 and 18 are 2 of the ligation reactions for comparison.

  • 17: SS_2_3
  • 18: NF_1_1
Programed PCR in thermocyclers 4,5,6. Called 2b12, 2b17, 2b22, and 2b27.
  •  (98°C 5 sec, 60°C 20 sec, 72°C 10 sec) X N cycles

9_22_15

It looks like 22 cycles is best, and worked on all samples so will be using that in the preparatory scale.

Ethanol precipitation

  • Set up an ethanol precipitation of all the broodstock samples I’ve extracted so far, as well as repeats of of the 4 samples used in the test scale PCR:
    • Population Sample Date extracted ng/uL Volume for 1 ug Volume sodium acetate Vol ethanol
      Oyster Bay BS_2_3 19.8 50.50505051 5.05 113.64
      Hood Canal BS_1_1 12.3 81.30081301 8.13 182.93
      Fidalgo BS_1_1 9.13 109.5290252 10.95 246.44
      Fidalgo BS_1_2 17.4 57.47126437 5.75 129.31
      Oyster Bay BS_2_6 23.4 42.73504274 4.27 96.15
      Oyster Bay BS_2_7 16.4 60.97560976 6.10 137.20
      Oyster Bay BS_2_8 16.8 59.52380952 5.95 133.93
      Hood Canal BS_1_5 12.1 82.6446281 8.26 185.95
      Hood Canal BS_1_6 23.5 42.55319149 4.26 95.74
      Hood Canal BS_1_7 14 71.42857143 7.14 160.71
      Hood Canal BS_1_8 22.8 43.85964912 4.39 98.68
      Hood Canal BS_1_9 13.9 71.94244604 7.19 161.87
      Hood Canal BS_1_10 27.7 36.10108303 3.61 81.23
      Fidalgo BS_1_4 8.9 112.3595506 11.24 252.81
      Fidalgo BS_1_5 18.1 55.24861878 5.52 124.31
      Fidalgo BS_1_6 16.1 62.11180124 6.21 139.75
      Fidalgo BS_1_7 35.8 27.93296089 2.79 62.85
      Fidalgo BS_1_8 22.7 44.05286344 4.41 99.12

      Left in ethanol and sodium acetate in -20C overnight.