Team:WashU/Notebook

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Notebook

You should make use of the calendar feature on the wiki and start a lab notebook. This may be looked at by the judges to see how your work progressed throughout the summer. It is a very useful organizational tool as well.

May 31

• Preliminary Shopping List

1. 1. PCR buffer w/o MgCl - 5ML - $45.00
   2. M8787- 5ML -MgCl Reagent- $49.30
   3. D7295-.5ML - dNTP - $73.00
   4. D4184-250UN - Taq Polymerase - $150.00
   5. D8045-250UN - AccuTaq - $300
   6. E1385-5ML – Ethidium Bromide – $23.70
   7. T8280-1L – Tris Acetate EDTA Buffer – $45.10
   8. NA1020-1KT – PCR Clean-Up Kit -$102.50
   9. NA1111-1KT - Gel Extraction Kit - $102.00

Subtotal: $890.60

• Met with Cohen Lab grad students to finalize plan and get cassettes.
• Received Leu2 cassette in pRS305 plasmid.
• Received Ura3 cassette in pRS306 plasmid.

June 1

• Lesson from Bert Berla on how to design primers
• Codon Optimized the four genes using tool at: http://www.encorbio.com/protocols/Codon.htm
  • Double checked gene and restriction sites to make sure enzyme does not cut in the middle of the gene
• Design Primers for cassettes
  • Ura3, Leu2, KanMX4, and NatMX4

June 2

• Made two liters of LB solution
  • 25g of LB Broth per Liter (10g Tryptone, 5g Yeast Extract, and 10g NaCl)
  • Autoclaved solutions: 30 minute sterilization.
  • Refrigerated after cooling.

June 3

• Made YPD

1. 1. In 800ml water in 1 L bottle dissolve 10g of BactoYeast extract
   2. Dissolve 20g of BactoPeptone in the above solution
   3. In 200ml water in 500ml bottle dissolve 20g Dextrose
   4. Autoclave both, combine after autoclaving. (30 minute sterilization)

• Made 1000X Ampicillin Stock
  • Added 2g Ampicillin to 20ml water.
  • Added NaOH until dissolved.
  • Sterile filtered.
  • Frozen in -20C Freezer

• Made cultures of E. coli strains with KanMx4 and Natmx4 inserts.
  • In culture tubes, added 5ml LB and 5ul 1000X Ampicillin Stock.
  • Transferred one colony per strain from plates to culture tubes.
  • Incubate at 30 degrees Celsius shaking at 225rpm overnight.

• Made cultures of Yeast strains BC177 and BC178
  • Added 5ml YPD to two culture tubes.
  • Transferred one colony per strain from plates to culture tubes.
  • Incubate at 30 degrees Celsius shaking at 225rpm overnight.

June 4

• Making freezer stocks of yeast cultures BC177 and BC178
  • Add 1.25mL glycerol to yeast culture
  • Freeze yeast culture in -80 degree freezer

• Make E.coli mini-preps for plasmids containing KanMX4 and NatMX4 (Sigma-Aldrich Mini-Prep Kit)
  • Transferred 4 ml of each culture to microcentrifuge tubes.
  • Centrifuge for one minute at 12000xg
  • Pour out supernatant
  • add 200uL of resuspension solution with RNase
  • add 200uL of lysis buffer
  • add 350uL of neutralization buffer
  • Centrifuge for 10 minutes at 12000xg
  • Insert a Miniprep Binding Column into microcentrifuge tubes and add 500uL of Column Preparation Solution to each miniprep column.
  • Centrifuge at 12000xg for 1 minute. Discard the flow-through
  • Take the lysis of the cultures resulting from the 10 minute centrifuge and pipet it into the binding column
  • Centrifuge at 12000xg for 1 minute. Discard the flow-through
  • Add 500uL of Wash Solution 1 to the column and centrifuge at 12000xg for one minute. Discard the flow-through.
  • Repeat the previous step
  • Add 750uL of Wash Solution 2 (with ethanol) to the column and centrifuge at 12000xg for one minute. Discard the flow-through.
  • Centrifuge at 12000xg for one minute.
  • Transfer the column to a fresh collection tube and add 100uL of Elution Solution to the column
  • Centrifuge at 12000xg for one minute.
  • Store the eluate at -20 degrees C

• This procedure was done separately for the plasmids that contain KanMX4 and NatMX4.

June 5

Read absorbances for all four solutions that contain plasmids with our cassettes: Ura3, Leu3, KanMX4, and NatMX4.

Data was obtained using a nano-drop spectrophotometer. Absorbance was observed between 250nm and 280nm.

DNA Concentrations were as follows:

• Ura3: Very high absorbance reading, must be diluted 1/10 in order to get accurate concentration reading.
• Leu2: Very high absorbance reading, must be diluted 1/10 in order to get accurate concentration reading.
• KanMX4: 30.5 ng/uL
• NatMX4: Very low absorbance reading, eluent was discarded.
• Last year's NatMX4 solution: Very high absorbance reading, must be diluted 1/10 in order to get accurate concentration reading.

• Made new culture of NatMX4
  • 5ml of TB + 5uL of 1000x Ampicillin
  • Incubated overnight at 31 degrees Celsius.

June 6

• LEU2 group
  • Make dilution for nanodrop
    • Make solution of 5uL LEU2, 45uL DI water
    • Concentration: 42.0 ng/uL

• URA3 group
  • Make dilution for nanodrop
    • Make solution of 5uL URA3, 45uL DI water
    • Concentration: 35.9 ng/uL

• KanMX4 group
  • 30.5 ng/uL (from previous day)

• NatMX4 group
  • Performed mini-prep on previous day's culture
  • 200uL eluent with concentration of 28.7 ng/uL
  • Made a 1/10 dilution of last year's NatMX4 stock. (DNA Concentration: 23.3 ng/ul)

June 7

• Ordered PCR materials and electrophoresis materials from Sigma-Aldrich.
• Designed primers to add homology to left side of cassette and an AvrII site to right side of cassette.
• Primer designs are:

Leu2

• Forward: TTT CCT AGG CCA AAC TGG AAC AAC ACT CAA CCC

• Reverse: ATA TTT AAT TAT TGT ACA TGG ACA TAT CAT ACG TAA TGC TCA ACC TAA TTT CGT GTC GTT TCT ATT ATG AAT TTC ATT TAT

Ura3

• Forward: TTT CCT AGG ACC ACA GCT TTT CAA TTC AAT TCA TCA TTT

• Reverse: AGT ATC ATA CTG TTC GTA TAC ATA CTT ACT GAC ATT CAT AAC CGC ATA GGG TAA TAA CTG ATA TAA TTA AAT TG

KanMX4

• Forward: TTT CCT AGG AGC TTG CCT CGT CCC CGC C

• Reverse:ATG AAC ATA TTC CAT TTT GTA ATT TCG TGT CGT TTC TAT TAT GAA TTT TCG ACA CTG GAT GGC GGC GTT

NatMX4

• Forward: TTT CCT AGG AGC TTG CCT CGT CCC CGC C

• Reverse: GGG TAA TAA CTG ATA TAA TTA AAT TGA AGC TCT AAT TTG TGA GTT TAG TCG ACA CTG GAT GGC GGC GTT

June 8

• Split into four technique groups

• PCR group
  • Practice PCR
    • Mastermix:
      • 10x buffer:10uL
      • betaine: 25 uL
      • dNTP: 2.0uL
      • Primer 1: 2.5 uL
      • Primer 2: 2.5 uL
      • Taq polymerase: 5 uL
      • dH20: 28.0 uL
    • Sample 1:
      • 3uL MgCl2
      • 1uL DNA template
      • 16 uL master mix
    • Sample 2:
      • 4uL MgCl2
      • 1uL DNA template
      • 15 uL master mix
    • Sample 3:
      • 5uL MgCl2
      • 1uL DNA template
      • 14 uL master mix
    • Sample 4 (Negative Control):
      • 4uL MgCl2
      • 15 uL master mix

94 degrees: 4min

34 Cycles:

• 94 degrees: 30 sec
• 58 degrees: 30 sec
• 72 degrees: 2 min (2kb product)

72 degrees: 5min

4 degrees: hold

Gel Team:

• We made a gel to use tomorrow:
  • 1. Added 500 mL 1xTAE and 5g Agarose
  • 2. Microwaved until dissolved completely
  • 3. Allowed to cool until able to handle and added 9 mL ethidium bromide
  • 4. Poured into gel mold and allowed to cool overnight

June 9

Gel Team:

• We ran the DNA the PCR team amplified yesterday
  • filled the electrophoresis chamber with 1xTAE
  • Added 2 mL loading buffer to each sample
  • put ladder and 4 samples into gel
  • ran electrophoresis for ~1h
• We imaged the gel
  • used UV imaging machine to take picture below
  • [[1]]

• The desired band was not visible. We determined the problem was we were testing the wrong template DNA

PCR team:

• We repeated PCR with new template DNA and freshly ordered supplies

Recipe per sample for running plasmid DNA:

• 2.5uL 10x buffer
• 1.25 uL dNTP
• 1.5 uL forward primer 44
• 1.5 uL reverse primer 43
• 16.5 uL dH20
• 0.25 uL Accutaq LA DNA polyermerase

Mastermix:

• 12.5uL 10x buffer
• 6.25 uL dNTP
• 7.5 uL forward primer 44
• 7.5 uL reverse primer 43
• 82.5 uL dH20
• 1.25 uL LA polyermerase

Sample 1, 2, 3:

• 1.5 uL DNA of plasmid pTCP2031v
• 23.5 uL Mastermix

Sample 4:

• 23.5 uL plasmid Mastermix

Recipe per sample for running genomic DNA:

• 2.5uL 10x buffer
• 1.25 uL dNTP
• 0.5 uL DMSO
• 0.5 uL forward primer 42
• 0.5 uL reverse primer 43
• 17.0 uL dH20

Mastermix:

• 12.5uL 10x buffer
• 6.25 uL dNTP
• 2.5 uL DMSO
• 2.5 uL forward primer 42
• 2.5 uL reverse primer 43
• 85.0 uL dH20
• 1.25 uL LA polyermerase
• 0.25 uL Accutaq LA DNA polyermerase

Sample 5, 6, 7:

• 1.5 uL vector DNA
• 23.5 uL Mastermix

Sample 8: 23.5 uL genomic Mastermix

Run same temperatures as before with 34 cycles

June 10