
The experiment was much the same as before. I added radiolabeled USS-1 fragments to either wild-type or rec-2 competent cell preps, incubated for 5 minutes, and then either prepared total DNA or did the periplasmic extraction (TE/1.5M CsCl + phenol/acetone, 1:1).
Since wild-type cells will take up the fragment, but also incorporate labeled subunits from degradation of taken up DNA, I can tell if the periplasmic DNA prep managed to exclude chromosomal DNA. But first, I counted the radiolabel present in the different cellular fractions...
This time, about a quarter of the USS-1 fragment added was taken up within five minutes (wild-type: 26%; rec-2: 28%). I suspect these numbers are lower than the last time I did it, because my five minutes was really five minutes (whereas the first time, I think I was 2-3 minutes late).
The extraction: When I collected the aqueous phase, I also collected the organic phase, and the interface between the phases (which should contain the cells minus their outer membranes). I counted the radiolabel in these different fractions as before:

But here's the important bit:

Lane 2: Total DNA, wild-type + USS-1 for 5 min.
Lane 3: Total DNA, rec-2 +USS-1 for 5 min.
Lane 4: Peri DNA, wild-type + USS-1 for 5 min.
Lane 5: Peri DNA, rec-2 +USS-1 for 5 min.
The important point here is that in the total DNA extract of wild-type, both intact donor USS-1 and chromosomal labeling are evident, while in the peri-extract of wild-type, there is no chromosomal label.
This means that the extraction I did successfully purified periplasmic DNA over chromosomal DNA. Fabulous!
Now I need to scale this protocol up, and get cleaner DNA (i.e. use RNase), so hopfully I can see this without using radiolabel. If I can really get clean periplasmic DNA with little or no chromosomal contamination, I will move onto doing the "real" experiment with donor DNA made up from sheared genomic DNA of another isolate.
Yay!
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