Difference between revisions of "Team:Warwick/Protocols"

Revision as of 13:16, 17 September 2015

Warwick iGEM 2015

Protocols

To ensure that our experiments went as smoothly and efficiently as possible, we followed tried and tested protocols.

Competent Cell Protocol

Produces chemically competent cells

IMPORTANT: Pre-cool all the buffers and tubes that you use to 4ºC – This will take many hours in a fridge, over an hour on ice, the fastest is to use an ice/water slurry.
1. Take a single colony from an LB agar plate, inoculate in 5 ml of LB broth and incubate for overnight, 200 rpm at 370C.
2. Dilute 200 µL of culture in 100 ml of LB broth and incubate with shaking until the culture reaches an OD value of 0.30-0.35. You can make larger volumes if you like.
3. Keep the culture on in ice/water bath for 30 min, mixing every now and again to ensure even cooling. Make sure the culture never warms above 4ºC from this point on.
4.Transfer to pre-cooled centrifuge tubes and centrifuge at 3000 rpm at 40C for 10 min.
5. Remove the supernatant, then resuspend the bacteria in 10 ml of 100 mM CaCl2, mix well and incubate for 30 min on ice.
6. Centrifuge at 3000 rpm at 40C for 10 min. Discard the supernatant, then add 10 ml of 100 mM MgCl2, mix then incubate for 30 min on ice.
7. Centrifuge at 3000 rpm at 40C for 10 min and add 2 ml CaCl2 with 10% glycerol, resuspend bacteria.
8. Transfer 50 µL of culture into pre-cooled 1.5mL eppendorf tubes (on ice, or do this in the cold room). Snap freeze cells in liquid nitrogen and transfer to -80 freezer.

Chemical transformation

Puts your plasmid into cells

1. Take chemically competent cells (-80C freezer) and thaw on ice/water mix.
2. Add plasmid DNA to 50uL of competent cells: for minipreps 0.5-1 uL of DNA is enough, for ligations, use 5-10 uL. Mix thoroughly.
3. Leave on ice for 30-45 minutes. Turn on the waterbath set to 42C, so it reaches the target temperature over this time.
4. Heat shock the cells at 42C for 30 seconds. This will create pores in the competent cells through which the plasmid can enter into the cell.
5. Put back on ice for 2 minutes. This allows the cell to recover and begin repairing the pores, preventing cell death.
6. Add 950uL of growth media (e.g. SOC, LB, etc.) bringing the volume up to ~1000uL
7. Incubate with shaking at 37C for 45-60 minutes.
8. Plate 200uL on appropriate antibiotic: If using a ligation (or anything likely to have low efficiency) centrifuge the cells first at 8000rpm for 2 minutes and resuspend in 200uL of media then plate everything. If there are still some cells left after plating, the rest can be kept up to 3 weeks in a 4 degree fridge.
9. Incubate overnight at 37C.

Ethanol Precipitation Protocol

Simple method for gel extraction

Ethanol Precipitation of DNA Reagents Needed:

• 3 M sodium acetate pH 5.2 or 5 M ammonium acetate
• DNA
• 100% ethanol

Extracting gel

After running a gel and identifying the band that contains the DNA that you wish to extract, simply use a scalpel to cut around the band leaving as little excess agarose gel as possible.

Protocol

1. Measure the volume of the DNA sample.
2. Add 1/10 volume of sodium acetate, pH 5.2, (final concentration of 0.3 M) - These amounts assume that the DNA is in TE only; if DNA is in a solution containing salt, adjust salt accordingly to achieve the correct final concentration.
3. Mix well.
4. Add 2 to 2.5 volumes of cold 100% ethanol (calculated after salt addition).
5. Mix well.
6. Place on ice or at -20 degrees C for >20 minutes.
7. Spin a maximum speed in a microfuge 10-15 min.
8. Carefully decant supernatant.
9. Add 1 ml 70% ethanol. Mix. Spin briefly. Carefully decant supernatant.
10. Air dry or briefly vacuum dry pellet.
11. Resuspend pellet in the appropriate volume of TE or water.

Double restriction digestion for NEB restriction enzymes

Cuts a select piece of DNA from a plasmid

Protocol

Set up the reaction as follows:
- 1ug DNA
- 5uL 10x digest buffer (use NEB cloner to find which buffer works best with which enzyme)
- 1uL or 10 units of first enzyme
- 1uL or 10 units of second enzyme
- Up to 50uL nuclease-free water

Incubate at 37C for 1 hour. If the enzymes being used are both time save qualified, this can be reduced to 5-15 minutes, but incubating for longer is still recommended.
Add the reagents into the mix from largest volume to smallest, always finishing with adding the enzymes in last.
If multiple restriction digests are being set up, a master mix containing everything but the sample DNA can be made with the condition that the concentrations of the different sample DNA are similar or equal.

Bacterial immunofluorescence protocol

For preparing slides to be visualised under fluorescent microscopy

1. For every cell type that needs testing, grow a culture of bacterial cells in 5mL LB (+antibiotics) overnight at 37 ˚C.
2. Next morning, take OD600 of the cultures (OD of 1 for E. coli corresponds to ~10^8 cells/mL), and dilute into 2 fresh 5mL LB tubes (+antibiotics) to OD600 of ~0.01. To one of these tubes, add IPTG to end concentration of 1mM. Incubate both tubes in a 37 ˚C shaker.
3. After ~3 hr of incubation, start monitoring OD of the cultures every half hour. We want to fix these cells at an OD600 of ~0.5.
4. As soon as a culture reaches OD600 of ~0.4-0.5, spin down 1mL of the culture in an Eppendorf tube at 8000xg (=rcf) for 1 min, and carefully discard the supernatant (be careful so as to only remove the supernatant, without disturbing the cells in the pellet).
5. Re-suspend the pellet in 1mL 1xPBS by pipetting up and down 5 times. Spin down the cells at 8000xg (=rcf) for 1 min, and carefully discard the supernatant.
6. Repeat the PBS wash in Step-5 two more times, but this time only use 0.5mL PBS.
7. Now, re-suspend the cells in 0.5mL 1xPBS by pipetting.
8. Mix 500 uL Blocking buffer with the annealed oligo (5.13uL) for each cell type in a separate Eppendorf tube, then add this to your cells.
9. Spin down the cells at 8000xg (=rcf) for 1 min, and carefully discard the supernatant.
10. Do 1x PBS wash (0.5mL PBS).
11. Now, fix the cells (in the tube itself) by resuspending in 1xPBS+4%(para)formaldehyde (we used glutaraldehyde but it fulfills the same purpose) (500uL). Incubate at room temperature for 20 min.
12. Do 1x PBS washes (0.5mL PBS)
13. Drop 50uL of the resuspension on a coverslip (round coverslips preferred), and incubate at 37 ˚C until it is completely dry. Once dry, save the coverslip at RT until all the cultures have been processed similarly.
14. Add a drop of the mounting medium (ProLong Diamond Antifade Reagent, Fisher #15372192) on a glass slide and place the coverslip on top of it (bacterial-side-down).
15. Seal the edges of the cover-slip with nail-polish, and save in the fridge (4˚C), for later visualization.

Design by Warwick iGEM 2015