REVISE FROM S11 M2
Last time you purified your 16S PCR product, reacted it with specially prepared DNA, and transformed the product into an engineered cell strain. Eight (?) independent colonies were selected from each of your plates and grown overnight in liquid culture. You will isolate and sequence DNA from each colony, then pool your results with all other groups studying that particular bird sample and construct a phylogenetic tree representing the bacterial composition in that sample.
Last time we talked about the features of the transformation strain to synthesize whole plasmid... now let's talk about those relevant to extracting DNA...
As you can see in the linked manual (PDF), these cells have the following genotype: recA1 endA1 gyrA96 thi-1 hsdR17 supE44 relA1 lac [F ́ proAB lacIqZΔM15 Tn10 (Tetr)]. Two gene mutations make XL1-Blue very useful "workhorse" cells for cloning. First, endA1 limits the non-specific destruction of plasmid (and chromosomal) DNA normally carried out by the EndA enzyme, thus maximizing DNA recovery. Second, recA1 makes the cells incapable of homologous recombination, which could otherwise cause undesirable intermingling between the plasmid and chromosomal DNA.
The procedure for DNA isolation at this scale is commonly termed "mini-prep," which distinguishes it from a “maxi-prep” that involves a larger volume of cells and additional steps of purification. The overall goal of each prep is the same--to separate the plasmid DNA from the chromosomal DNA and cellular debris, allowing the plasmid DNA to be studied further. In the traditional mini-prep protocol, the media is removed from the cells by centrifugation. The cells are resuspended in a solution that contains Tris to buffer the cells and EDTA to bind divalent cations in the lipid bilayer, thereby weakening the cell envelope. A solution of sodium hydroxide and sodium dodecyl sulfate (SDS) is then added. The base denatures the cell’s DNA, both chromosomal and plasmid, while the detergent dissolves the cellular proteins and lipids. The pH of the solution is returned to neutral by adding a mixture of acetic acid and potassium acetate. At neutral pH the SDS precipitates from solution, carrying with it the dissolved proteins and lipids. In addition, the DNA strands renature at neutral pH. The chromosomal DNA, which is much longer than the plasmid DNA, renatures as a tangle that gets trapped in the SDS precipitate. The plasmid DNA renatures normally and stays in solution, effectively separating plasmid DNA from the chromosomal DNA and the proteins and lipids of the cell.
Normally in 20.109 we do an in-house mini-prep procedure according to the steps above followed by ethanol precipitation. However, because we are working with a low-copy plasmid, today we will use a commercially available kit to give you the best chance of success. The principle is the same as that of our "quick and dirty" (and cheaper!) prep, but is combined with the silica gel column purification you are familiar with from using other Qiagen kits.
Miniprepped DNA will be sent for sequencing...
You will figure out which clone to use by analyzing your sequencing data.
Normal bases versus chain-terminating bases
The invention of automated sequencing machines has made sequence determination a relatively fast and inexpensive endeavor. The method for sequencing DNA is not new but automation of the process is recent, developed in conjunction with the massive genome sequencing efforts of the 1990s. At the heart of sequencing reactions is chemistry worked out by Fred Sanger in the 1970s which uses dideoxynucleotides (see schematic above left). These chain-terminating bases can be added to a growing chain of DNA but cannot be further extended. Performing four reactions, each with a different chain-terminating base, generates fragments of different lengths ending at G, A, T, or C. The fragments, once separated by size, reflect the DNA’s sequence. In the “old days” (all of 15 years ago!) radioactive material was incorporated into the elongating DNA fragments so they could be visualized on X-ray film (image above center). More recently fluorescent dyes, one color linked to each dideoxy-base, have been used instead. The four colored fragments can be passed through capillaries to a computer that can read the output and trace the color intensities detected (image above right). Your sample was sequenced in this way on an ABI 3730 DNA Analyzer.
Analysis of sequence data is no small task. “Sequence gazing” can swallow hours of time with little or no results. There are also many web-based programs to decipher patterns. The nucleotide or its translated protein can be examined in this way. Thanks to the genome sequence information that is now available, a new verb, “to BLAST,” has been coined to describe the comparison of your own sequence to sequences from other organisms. BLAST is an acronym for Basic Local Alignment Search Tool, and can be accessed through the National Center for Biotechnology Information (NCBI) home page.
In another week you will finally get to see the results of all your hard work...
Part 1: Extract DNA from selected clones (mini prep)
Each partner today has eight(?) minipreps to do. You may find it easier to complete the sixteen(?) total minipreps in two shifts than to attempt to "quickly" pipet across sixteen samples. Is there a place for using the multichannel here? Every other one filled? Tricky with epps.
- Pick up your eight(?) candidates cultures, which are growing in the test tubes labeled with your team color. Label eight eppendorf tubes to reflect your candidates (C1-8).
- Vortex the bacteria and pour ~1.5 mL of each candidate into an eppendorf tube.
- Balance the tubes in the microfuge, spin them at maximum speed for two minutes, and remove the supernatants with the vacuum aspirator.
- Pour another 1.5 mL of culture onto the pellet, and repeat the spin step.
- Resuspend the cell pellet in 250 μL buffer P1.
- Buffer P1 contains RNase so that we collect only our nucleic acid of interest, DNA.
- Add 250 μL of buffer P2 and mix by inversion until the suspension is a homogeneous blue color. About 4-6 inversions of the tube should suffice. You may incubate here for up to 5 minutes, but not more.
- Buffer P2 contains sodium hydroxide for lysing.
- The blue color comes from a special reagent that is not required for purification, but is simply used to check one's mixing technique.
- Add 350 μL buffer N3, and mix immediately by inversion until there is no blue colour (4-10 times).
- Buffer N3 contains acetic acid, which will cause the chromosomal DNA to messily precipitate; the faster you invert, the more homogeneous the precipitation will be.
- Buffer N3 also contains a chaotropic salt in preparation for the silica column purification.
- Centrifuge for 10 minutes at maximum speed. Note that you will be saving the supernatant after this step.
- Meanwhile, prepare 8 labeled QIAprep columns, one for each candidate clone, and 8 trimmed eppendorf tubes for the final elution step.
- Transfer the entire supernatant to the column and centrifuge for 1 min.
- Wash with 0.5 mL PB, then separately with 0.75 mL PE, with each spin step 1 min long.
- After removing the PE, spin the mostly dry column for 1 more min.
- It is important to remove all traces of ethanol, as they may interfere with subsequent work with the DNA.
- Add 30 μL of pH 7 water to the top center of the column, wait 1 min, then spin 1 min to collect your DNA.
Part 2: Measure DNA concentration
Part 3: Prepare sequencing reactions
For each miniprep, you will prepare two sequencing reactions...
Part 4: Count colonies
Part 5: Sensitivity/specificity analysis for microsporidia primers
For next time
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