IGEM:Harvard/2006/Cyanobacteria/Notebook/2006-7-18

DNA Miniprep of topo+kaiabc clones

With the Topo prepared clones in e.coli Hetmann created:

 1: kaiabc+topo #1
 2: kaiabc+topo #1
 3: kaiabc+topo #1
 4: kaiabc+topo #1
 5: kaiabc+topo #2
 6: kaiabc+topo #2

I aliquoted 4mL of each topo clone into its seperate vial and conducted a DNA miniprep based on the Qiagen miniprep kit 6/05 handbook p22-23. Used old Qiagen miniprep kit (had very little P2 buffer in it); new one did not have RNAase added. #1,4,and 5 did not have as many cells as 2,3, and 6. Used centrifuge for the large centrifuge tubes; 4.4k for 10 min.

note: tubes 4,5,6 may have been a bit contaminated by either 1,2, or 3; during loading of first centrifuge, but most likely okay.

The final reactions are stored in blue 1.5 tubes marked (number, kaiabc topo DNA). used 30 uL extraction.

DNA nanodrop data:

  1: 153.3 ng/uL
  2: 14.0 ng/uL
  3: 14.4 ng/uL
  4: 8.9 ng/uL
  5: 12.5 ng/uL
  6: 27.2 ng/uL

Weirdly enough, sample 1 and the other ones fell within 260/280 as 1.8-2.0... did NOT dilute sample 1.

Storage of topo+kaiabc clones

For all 6 topo clones, I aliquoted 666uL of each into a cryogenic vial, and added 666uL of 50% glycerol. Each is in a vial at -80C, in a cap with blue writing and dated.

Digest of the topo+kaiabc clones and the one we were using the past week

In order to do a pre-sequence test to see if our template is correct, I did a restriction digest using the pstI enzyme. Based on this Media:Pcr2topoblunt.pdf file, if we cut at the pst1 site only we can do three diagnoses. The following is what I look to test.

• 1. If there is no kaiABC in the vector, we will get a 3519 bp fragment.
  2. If there is no kaiABC in the vector and kaiABC freeflowing, we will get a 500 bp fragment, a 2390bp fragment, and a 4519 bp fragment
  3. If there is kaiABC in the vector, we will get a 2390bp fragment and a 4138bp fragment
  4. If there is random crap in the vector, the bands will be different; a 3kb band prehaps?
  5. Positive control: reactions itself?
  6. Negative control: no DNA

Granted, using SpeI or double digesting may provide more info, but I think we're out of SpeI and ... yeah.

Per reactions 2,3,4,5,6 the amount in a 50uL rxn (gives ~140-270ng of DNA/rxn depending on concentration):

  10uL DNA
  5uL 10x Buffer3
  1uL PstI
  0.5uL 100x BSA
  33.5uL dH20

For reaction 1 the amount in a 50uL rxn (gives 300ng of DNA):

  2uL DNA
  5uL 10x Buffer3
  1uL PstI
  0.5uL 100x BSA
  41.5uL dH20

For reaction "Tp" the amount in a 50uL rxn (gives 300ng of DNA, was template we were using last week):

  5uL DNA
  5uL 10x Buffer3
  1uL PstI
  0.5uL 100x BSA
  38.5uL dH20

For negative:

  5uL 10x Buffer3
  1uL PstI
  0.5uL 100x BSA
  43.5uL dH20

Master Mix was preformed for all samples: combining BSA, Buffer3, PstI, and dH20.

The run time is:

 37C for 6 hours
 80C for 20 minutes
 4C for forever

The run is being done on the PCR machine #1. Will be done by 1030AM 7/18.

Repeat of colony PCR (see 7/10)

Assuming that our digests are not turning out good, I repeated the colony PCR step from cyanobacteria. Biggest change here is the use of solid monocolonal colony intstead of liquid polyclonal. Lysing by thermocycler @ 95C @ 5min.

The protocol is:

1 experimental, 1 negative (no template), and 1 BB test.

The experimental/negative had:

  5uL/0uL colony DNA
  1.5uL 20mM dNTP (new)
  1.0 uL extR
  1.0 uL extF
  0.5uL HotStarTaq (N)
  5uL 10x buffer
  41.5/46.5 dH20

The BioBricks test, which looks for contamination in the primers, had:

  1.5uL dNTP
  1.0 uL RF
  1.0 uL (reverse)
  1.0 uL HotStarTaq (N)
  5 uL 10x buffer
  41.5uL dH20

They are in 0.2mL miniPCR tubes in PCR#6. (3 samples total) Tops in blue.

Repeat of 7/17 transformation

I (Jeff) plated the yesterday's transformants on the wrong plates, so I redid the Topo ligation and transformation. I used 30 µL, 15 µL, and 15 µL of competent cells for the experimental, negative, and positive controls.

I plated the transformants on 6 plates (1 negative control, 1 positive control, 4 experimental) at around 1 PM.

Gels