General Protocols

Agarose Gel Electrophoresis

1. Add TAE Buffer (100 mL) and Agarose (1g) to a flask [for a 1% gel]
2. Cover with plastic wrap, poke hole in top. Then microwave flask until agarose is fully dissolved; avoid boiling
3. Take flask to fume hood, and allow to cool to touch. Add REDsafe (4 μL) to agarose, gently swirl to mix
4. Gently pour agarose into assembled gel casting tray, removing any bubbles with a pipette tip
5. Allow gel to solidify until translucent. Then transfer to running apparatus filled with TAE buffer
6. Load samples containing 3 μL loading dye and ~10-15 μL of DNA
7. Run gel at 110V until the dye is ~2/3 of the way down the gel (approx. 40 mins)

Preparing Chemically Competent E. coli Cells

1. Inoculate 5-10mL LB with Top10 E. coli culture at 37°C shaking over night
2. Subculture 1mL of bacteria into 50mL LB at 37°C shaking until OD₆₀₀ is 0.4-0.6 (~2.5 hr)
3. Centrifuge the subculture at max for 20 min at 4°C
4. Resuspend pellet in 12.5mL cold CaCl₂ (50mM, 15% glycerol)

Preparation of Antibiotic Agar

• LB agar
• Plates
1. Weigh 35g of LB-Agar powder mix per litre of media desired. One litre makes 40-50 plates. Ensure that that the mixture volume does not exceed half of the volume of the flask/contained used, as it will boil over in the autoclave.
2. Dissolve LB-Agar, using water from one of the wall mounted Nanopure filters. Add a stir bar and use a magnetic stirrer to facilitate mixing.
3. Cover the flask with aluminum foil, and secure the foil with autoclave tape. The foil should be somewhat loose (to avoid building pressure in the flask while sterilizing and blowing the foil off), but not so loose that lots of liquid can escape.
4. Put the flask in a plastic autoclave tray, load into the autoclave, and sterilize using the 20 minute liquid program.
5. Once the autoclave finishes venting (which can take twice as long as the sterilization proper), check that the foil covering is still in place. If it is not, the media is contaminated! Unload using the insulated oven gloves.
6. Allow the media to cool until it can be handled without the oven mits. The cold room can be used to speed this up. Alternatively, if a large batch of media is prepared flasks may be kept hot in the prep lab water bath, to avoid all of them cooling at once. Agar polymerization cannot be reversed once it starts, but media can be kept from solidifying by keeping it hot.
7. Once media is cool, add other desired ingredients. Use the magnetic stirrer to mix, but do NOT add a stir bar now, or the media will be contaminated. (If one wasn't added before, you must do without.)
8. Pour agar into plates
Common additions include:
1. Ampicillin (stock 100mg/ml, final 100μg/ml)
2. Kanamycin (stock 50mg/ml, final 50μg/ml)
3. Chloramphenicol (stock 50mg/ml, final 10μg/ml)
4. To achieve final concentrations, add 1mL of stock per 1L of media, except for chloramphenicol, where 0.6mL per 1L of media is added instead.
5. Pour directly from the flask into sterile petri plates. Use a quick pass with a Bunsen burner flame to eliminate any bubbles that form during pouring. Do not subject the plate to continuous heat or the plate will melt, and the heat sensitive ingredients added in the previous step will be destroyed. Bubbles can allow cells to access nutrients without being exposed to the plate's antibiotic, and should be blown out immediately before the gel can set. It's a good idea for one person to pour while another flames bubbles.
6. Allow the plates to stand right side up overnight, or until the gel sets if they are needed sooner. Plates should be stored upside down to prevent condensation from falling on the media. Store petri plates in the plastic bags they ship in, in the 4 degree cold room.
Overnight Cultures (per culture tube)
• 10mL culture tube (16mm x 160mm or 16mm x 125mm) or 15mL Falcon tube
• 5mL LB
• 5μL 1000X antibiotics
• Single colonies on a plate (best not to start an overnight from a glycerol stock)
1. Add 3mL sterile/autoclaved LB in a 15mL Falcon tube
2. Pipet 3μL of 1000X antibiotic into the LB
3. Select a single colony using a sterile toothpick or pipette tip
4. Place toothpick or pipette tip in the culture tube and stir
5. Remove toothpick, or in the case of a pipette tip, leave in the tube
6. Place culture tube in incubator at 37°C overnight shaking vigorously (250 RPM)
Glycerol Stocks
• Overnight bacterial growth
• Screw cap tubes
• Glycerol
1. Pipet 0.5mL of glycerol into two 1.5mL screw cap tubes
2. Add 0.5mL of overnight culture to each tube
3. Pipet up and down to gently mix
4. Place one tube in -20°C freezer
5. Place the other tube in -80°C freezer
Plating a liquid culture onto agar
• Agar plate
• Liquid bacterial culture
• 100% ethanol
• Plating rod
1. Suspend culture in ~100uL of LB media to produce concentrated liquid culture
2. Pipette liquid culture onto antibiotic agar plate
3. Dip plating rod into ethanol and burn any excess fluid. Cool rod on agar, making sure to avoid bacteria
4. Use plating rod to evenly spread the liquid culture throughout the plate.
5. Sterilize plating rod in between each plate
6. Store plates in 37°C incubator until adequate bacterial growth is observed.
Streaking plates
• Agar plate
• Streaking loop
1. Touch desired colony with a sterilized streaking loop until adequate sample is acquired
2. Gently streak onto surface of agar plate in a zig-zag motion until 1/4 of the plate has been streaked
3. Sterilize streaking loop with fire until glowing hot
4. Repeat streaking motion on other 1/4 of plate
5. Sterilize and streak until entire plate is covered in a circular direction. Do not let the last two streaking patterns come into contact.
6. Place in 37°C incubator until adequate bacterial growth is observed.
7. When picking colonies from streaked plate, take advantage of the gradient in colony density and use only isolated colonies