20.109(S07): TA's notes for module 1

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M13 Redesign Module


General notes

Before term begins:

  1. Check that insert tag sequences make sense
  2. Streak out NB251 (M13K07) and NB257 (M13K07 with PstI site) on LB+Kan. Make 10 overnight cultures (2-3 ml LB+Kan 1000:1) of each or 20 of NB257 since it works for either BamHI or PstI. Miniprep these for the vector DNA the next day. Resuspend each pellet in 50 ul H20 and pool. Store at -20°. These will be used as cloning backbone starting on Day 1 of module.
  3. Double-check volume of NO150/151 and NO154/155 for c-myc cloning.
  4. NEB titers M13K07 on their strain ER2267 cat#E4103S. This strain is in the lab collection as NB271. Streak out a plate on LB+Kan so you will have colonies to pick for liquid cultures before phage titration. The Kan is important to select for the F'.
  5. Autoclave several racks of small and large test tubes.
  6. Make 1L top agar, divide between autoclaved 250 ml bottles, 100 ml per bottle for reheating
  7. Check volume/availability of needed kits, reagents:
    • M13K07 from NEB
    • restriction enzymes (PstI, ??)
    • Qiagen kit for agarose clean-up
    • T4 DNA ligase and buffer for ligation mix
    • super competent XL1-blue cells
    • Miniprep solutions
    • Protein gels
    • Anti-myc antibody

Daily Notes

Notes:Day 1

Before lab:

  1. Need to have backbone for restriction digest, made from miniprep of NB251 and NB257

Day of lab:

  1. No quiz on day 1
  2. Keep cold:
    • PCR tubes with 10 ul BamH1, PstI
    • NEB buffers 2,3 on ice
  3. Remember to freeze away digests (-20C) before leaving lab for the night.

Notes:Day 2

Before lab:

  1. Need to set up ER2267 (NB271) so there will be cells for 1.2 ml/group. Plate on LB+Kan, then overnight 3 ml LB + Kan in tubes.
  2. Need to pour 3 x 100 ml agarose gels for each day of lab, using one 10-well comb (thicker teeth) in each gel.
  3. Pour LB plates (2L), 6 plates per group, x 2 days
  4. Need top agar prepared
  5. Double-check volume of NO150/151 and NO154/155 for c-myc cloning.
  6. Check for phage stocks: M13K07 and another M13 phage called E4
  7. Check reagents and tubes in PCR Cleanup Kit
  8. Need 1kb ladder and loading dye

Day of lab:

  1. Need quiz
  2. Put gels in boxes for running, remove combs, add ~500 ml 1X TAE
  3. Need to melt 30 ml of top agar/group. Microwave in water bath for 2', invert to distribute any unmelted parts, heat another minute. (SC: I microwaved 1', swirled, microwaved 30", and it was melted, then into 55C water bath) It's very important that the top agar be fully melted for the students. Store molten in 55-60°C water bath.
  4. Bacterial overnights out
  5. Pipetmen, 5 ml pipettes and 50C water baths for phage plating
  6. Mix up equal volumes of oligos for gel control, then load 5 ul + 0.5 ul loading buffer in one lane of each gel
  7. 1 PCR tube/group
  8. Need 6 LB plates/group taken out of -20C and 6 small sterile test tubes/group.
  9. 20 ml sterile water in a few 50ml conical tubes
  10. Aliquot E4 and M13 phage stocks for dilutions, ~200 ul
  11. Need Qiagen kit for gel cleanup. Do not put out any reagents that are incomplete (e.g., do not put out PE that does not have ethanol added to it).
  12. Freeze purified backbone and annealed inserts, make sure all phage plates are in incubator.

Notes:Day 3

Before lab:

  1. Have LB-Kan plates poured. Need 5/group = 60, 1L makes 30-40 plates, so need to make a couple liters.
  2. Refill burners and jars with 100% ethanol

Day of lab:

  1. Need quiz
  2. Keep cold
    • 70% ethanol, 6 x 1.5 ml (full microtubes)
    • 100% ethanol, 6 x 1 ml
    • From -20°C freezer:
      • students' inserts and backbone
      • T4 DNA ligase, 3 aliquots in PCR tubes in cold-boxes
      • T4 ligase buffer, has ATP so must be kept cold
      • BamHI, PstI, 2 aliquots in PCR tubes in cold-boxes
      • NEB Buffers 2,3
      • aliquots of yeast tRNA from 109 Antibodies box
    • only take out of -80°C freezer when first group is ready, competency decreases with time on ice
      • super competent XL1-blue cells, one 200 ul aliquot per group
  3. Sodium acetate 3M, 6 x 100 ul in microtubes
  4. LB media, 10 ml per group, put in 50 ml conical tubes (3 x 30)
  5. Sterile water, 6 x 1 ml in microtubes for ligation and resuspending DNA
  6. LB-Kan plates out of 4C
  7. Kanamycin, 10 ul per group (2 tubes of 50 ul), keep cold
  8. large test tubes (4/group), 5 and 10 ml pipettes
  9. ice buckets for competent cells
  10. After incubating xformation plates for one day, blow colony plugs into overnights for use on Day 4. Students will have labelled tubes.

Notes:Day 4

Before lab:

  1. Make 2L 1X TAE for gels and running buffer
  2. Pour 3 1% TAE gels + EtBr 100ml with 2 10-tooth combs
  3. Aliquot solutions (see below)

Day of lab:

  1. Need quiz
  2. Aliquot solutions for miniprep (Solutions 1, 3, NaOH and SDS) for each group so stocks don't get contaminated.
    • Each group needs:
      • 400 ul Solution 1 (6 microtubes of 1000 ul)
      • 500 ul SDS 2% (6 microtubes of 1000 ul)
      • 500 ul 0.4M NaOH (6 microtubes of 1000 ul)
      • 600 ul Sol 3 (6 microtubes of 1000 ul)
      • 4 ml 100% Ethanol (6 x full 15 ml tubes)
      • 2 ml 70% Ethanol (6 x ~10 ml in 15 ml tubes)
      • sterile water bottle for each group
  3. Keep cold:
    • buffers
    • restriction enzymes
  4. ice buckets (one per bench should be fine, just for miniprep)
  5. 1 ml serological pipets for alcohols (optional)
  6. loading dye for gels

Notes:Day 5

Day before lab:

  1. Start overnights of 7x NB271 liquid cultures for plaque assay (3 ml of LB+Kan in large tubes), each group needs 1.2 ml cells
  2. Pour 2L of LB plates
  3. Have protein gels and chambers
  4. myc positive control NB269: streak on LB+Amp plate, have liquid LB+Amp cultures grown overnight for lab
  5. For each day, make microtubes of 1X sample buffer without BME (500 ul 2X + 400 ul H20) and of 500 ul 2X, add 100ul of BME to both on day of lab (could parafilm after adding BME, save 2 days)
  6. Make 3 L of transfer buffer for each day and refrigerate
  7. Make 1L 1X TBS-T in graduated cylinder, refrigerate, mix in 5% powdered milk close to lab day
  • Note: 2nd ab is goat antimouse GAM-AP in ab freezer box

Day of lab:

  • Need quiz
  • Turn on water baths and melt top agar
  • Protein gels and blot
  1. Students' candidates in liquid culture tubes
  2. Overnights of myc+ ctrls (1 ml aliquots)
  3. LB blank for spec
  4. Sample buffer + 100 ul BME, 2X and 1X tubes
  5. Lid locks for microtubes in hood
  6. Boiling tank on hot plate in hood with boiling chips
  7. 3 protein gel chambers with 2 gels each, set up
  8. M13K07 phage from sup bottle, 25 ul/gel
  9. "Kaleidoscope" protein molecular weight standard, in -20C in enzyme rack, aliquot 50 in microtubes, denature i
  10. Running buffer, 1X TGS made when needed, 1L/chamber, 10X above sink
  11. Transfer cassettes, ScotchBrite pads, filter paper, nitrocellulose
  12. Western transfer buffer, 1L/tank so 3L/day
  13. ice packs for Western
  14. Blocking buffer TBS-T + 5% milk, 50 ml/group
  15. Protein gels will have duplicate lanes so that blot can be cut in half. One half probed with anti-myc, the other anti-p3 or -p8 (new anti-p8, not tried yet). Figure out dilution of anti-p8??. Myc + control works.
  • Plaque assay
  1. top agar, melted in microwave and kept in 55C water bath
  2. 200 ul x 6 /group NB271/ER2267 bacteria for plaque assay
  3. 10^6 dilution of positive phage control in microtube
  4. small sterile test tubes, 6/group
  5. 6 LB plates/group for plaque assay (no phage, + phage control, 4 dilutions supernatant: 10^0,2,4,6)
  6. 5 ml pipets and Pipetmen

Notes:Day 6

  • EHS rep will come in and talk about cell culture work during first Western incubation period.
  • Talk about M13 refactoring during other incubation

Day of lab:

  1. Don't need quiz.
  2. First drafts of papers due at beginning of class via e-mail.
  3. Don't know if myc added is detectable??
  4. 12 small tupperware containers during class
  5. TBS-T, ~300 ml / group for rinsing/washing blots
  6. 6 x 30 ul of anti-myc antibody
  7. 6 x 15 ul of anti-p8 or anti-p3 antibody (trying 1:1000 due to lack of anti-p3 material)
  8. 30 ml / group (1:1000 Goat-Anti-Mouse-Alkaline Phosphatase) in TBS-T + secondary antibody
  9. 25 ml / group developing solution for AP, 1 ml 25X developing solution (in 4°C) + 24 ml MilliQ water, students add 250 ul of each of two solutions from kit in -20°C
p8 ab info
p3 ab info


  1. LB: 10 g Tryptone, 5 g Yeast Extract, 10 g NaCl per liter. 20g of Agar for plates. Autoclave 30 minutes with stirbar. Pour when ~55°. Let plates dry ON on bench and store in sleeves in 4°.
  2. Top Agar: 10 g Tryptone, 5 g Yeast Extract, 10 g NaCl, 1 g MgCl2*6H20 7 g Agar per liter. Autoclave then aliquot to 50 ml conical tubes or bottles. Store at RT. Melt in microwave in beaker of water, 2’ then keep molten in 55° water bath.
  3. Amp: 100 mg/ml in H20. Filter and store at 4°. Use at 1:1000 in liq media. 2ml/L in plates
  4. Tet: 20 mg/ml MeOH. Keep in dark at 4°. Use at 1:1000 in liq media. 1ml/L in plates
  5. Kan: 25 mg/ml in H20. Filter and store at 4°. Use at 1:1000 in liq media. 2ml/L in plates.
  6. Soln I for miniprep: 2.3 ml 40% glucose, 2.5 ml 1M Tris 8, 2 ml 0.5M EDTA. To 100 ml with good H20. Store at RT
  7. Soln II for miniprep: equal parts 2% SDS (2g/100 ml H20): 0.4M NaOH (1.6g/100 ml H20). Store components at RT. Mix just enough just before using.
  8. Soln III for miniprep: 29.4 g KAc dissolved in 60 ml H20. Add 11.5 ml glacial acetic acid. Bring to 100 ml final volume. Store at RT.
  9. DNA gel: 1% agarose gel in 1X TAE, 1 g agarose, 10 ml 10X TAE, 90 ml water, 2 ul EtBr
  10. Loading dye for agarose gel: 250 ul 1% XC (xylene cyanol), 750 ul 40% glycerol, 10 ul RNase. Store at RT.
  11. 5X TBE 5.4% Tris base, 2.75% Boric Acid, 10mM EDTA, pH 8.0
  12. 2X sample dye for protein gel (no BME): 4 ml 10% SDS, 5 ml 40% glycerol, 1 ml 1M Tris 6.8, 0.5 ml <1% bromophenol blue, stocks on NK's bench
  13. 1X sample dye for protein gel: 500 ul 2X sample dye, 400 ul H2O, 100 ul BME
  14. Running Buffer: 1X TGS (10X from BioRad: 161-0772)
  15. Western Transfer Buffer: 3.03 g Trizma base, 14.4g glycine, 200 ml methanol to 1L with good H20. Store at 4°C. (25 mM Tris, 192 mM glycine, 20% v/v methanol)
  16. TBS-T: Dilute 100 ml 10X TBS with 900 ml H20 then add 10 ml 10% Tween20
  17. TBS-T + 5% milk: add 2.5g milk powder to 50 ml TBS-T per blot.