Methods

Inserting the BBa_K977000 pyruvate kinase gene into BBa_K125000 vector required a number of different steps and techniques.

Because the vector already contained a usable promoter, the main procedure involved four different methods.

• Using site-directed mutagenesis to remove a naturally-occurring PstI restriction site in the pyruvate kinase gene
• Using PCR to “flank” the pyruvate kinase gene with the BioBrick Standard Restiction Enzyme sites
• Using 3A Assembly to insert the new part into the BBa_K125000 vector
• Transforming the cyanobacteria

SITE-DIRECTED MUTAGENSIS
Site-directed mutagenesis is a method for altering the sequence of DNA and can be used to produce both point and frame-shift mutations. In this case, it was possible to take advantage of codon redundancy and alter the DNA sequence without altering the amino acid sequence. It was necessary to do site-direct mutagenesis because the pyruvate kinase gene contains in its sequence two PstI restriction sites.
Because PSTI is part of biobrick assembly, it was necessary to use site-directed mutagenesis to remove these sites prior to cleaving and ligating the part. Otherwise PstI would chop the gene to pieces whenever we (or anybody else) tried to assemble anything with it.
Primer design was very simple, as the primers were identical to the gene except that they contained the desired mutations. Again, the primers were about 20 bp to ensure that they would only attach to one region along the gene.
Forward primer
Template strand- 5’- ctcatctccctgcaggtgaagcag 3’
Primer -5’- ctcatctccctccaggtgaagcag 3’
(Restriction sites are in red, point mutation is in blue)
Reverse primer
Again, the reverse primer necessitated the use of the reverse compliment of the original sequence.
Template strand 5’- CTGCTTCACCTGCAGGGAGATGAG -3’
Primer 5’- CTGCTTCACCTGCAGGGAGATGAG 3’

PCR
In order to get the pyruvate kinase gene to conform to Biobrick Standards, it was necessary to add the four Biobrick restriction sites.
This was done with a variation on PCR annealing and extension per the instructions given by the Registry. Theoretically, this method was simple. All it required was forwards and reverse primers that consisted of the BioBrick prefixes and suffixes and the first twenty base pairs of the gene.
Forward primer
5’- GTTTCTTGGAATTCGCGGCCGCTTCTAGATG TCAAAGTCCCACAGTGAAGC -3’
Reverse Primer
To orient the sequence 5’-to-3’, it was necessary to use the reverse compliment of the last twenty base pairs of the gene.
5’- GTTTCTTCCTGCAGCGGCCGCTACTAGTA TTATTACGGGACGGGCACCACGCGCA -3’
(Red is the tails, green is the gene)
After this, it would be possible to proceed with PCR as normal, and though the region of restriction sites would “hang off” in the first round of PCR, they would be added to the gene as “flanks” in subsequent rounds as the extension stage would transcribe the flanks on as well as the gene’s DNA. However, a number of challenges presented themselves.
At 51 and 55 bp, the length of the primers far exceeded the typical 40-45 bp. The long “free ends” that contained the restriction sites threatened to rip the section of matching sequence away from the template strand. It proved impossible to shorten these primers while still including the standard restriction site. Nonetheless, the primers were ordered and the experiment was attempted.
In the event of the failure of these super-long primers to anneal properly, it would also be possible to construct the restriction site flanks through multiple rounds of PCR, though this would be more time-consuming.

GIBSON ASSEMBLY
TIt would have also been possible to construct the PCL-5 gene entirely from oligos using Gibson assembly. The artificial synthesis of the approximately 1500-bp gene would require four oligos of single-stranded DNA. The ends of these oligos would contain small section of overlapping sequence, and could be annealed together, with DNA polymerase and DNA ligase completing and sealing the double strand. After this point, it would be possible to proceed with standard PCR.
The primary advantages of Gibson assembly included the fact that it would be possible to build the BioBrick restriction sites and altered PstI sites into the oligos. This is far simpler than using site-directed mutagenesis and PCR; however, ordering (and waiting for the synthesis of) such long oligos would actually be more time-consuming than using PCR and site-directed mutagenesis.

TINKER CELL
A program called TinkerCell was utilized to help visualize the steps taken through glycolysis and the fatty-acid pathway to create alkanes. The image created in TinkerCell allows one to see each step in the modification of a molecule. Beginning with glucose and ending with alkanes, the image shows what the molecule becomes, which enzyme catalyzes the reaction, what type of reaction occurs, what is required for the reaction to occur, and the other products of the reaction.

ASSAY FOR PYRUVATE KINASE ACTIVITY
Photosynthetic microbes, like cyanobacteria, hold the potential to produce biofuel with only sunlight and adequate growing conditions. These microbes do not need much space or require nutrient input to create fuel. However, biofuel output through this method is relatively low, which sparked our interest.

Whether it is diesel fuel or gasoline, most of the energy comes from alkanes. A cell makes alkanes by the fatty-acid pathway. A main resource needed for the fatty-acid pathway, acetyl-CoA, is produced by glycolysis. We hypothesize that if we increase the resources required for the production of alkanes, then the cell will produce more alkanes.

By overexpressing the catalytic protein pyruvate kinase, we hope to increase pyruvate within the cell. This should allow for an increase in activity within the alkane fatty-acid pathway because of pyruvates conversion to acetyl-CoA.

PEP phosphorylates ADP  1 molecule pyruvate + 1 molecule ATP


To determine the amount of pyruvate activity produced by our cyanobacteria (engineered for overexpression of pyruvate kinase), we must assay for pyruvate kinase. A cocktail of magnesium chloride, ADP, EDTA, bicine (buffer), NADH and lactate dehydrogenase is made. Added to the purified pyruvate from the cyanobacteria plus PEP, the lactate dehydrogenase will utilize the NADH to reduce pyruvate to lactate. The amount of lactate produced indicates the output of pyruvate from the cell and can be read using a spectrophotometer at 340 nm. Using the spectrophotometer readings and a mathematical formula that takes into account dissociation rate of PEP into pyruvate into lactate acid, our initial pyruvate amount is determined.

ASSAY FOR ALKANES
Whether it is diesel fuel or gasoline, most of the energy comes from alkanes. A cell makes alkanes by the fatty-acid pathway. A main resource needed for the fatty-acid pathway, acetyl-CoA, is produced by glycolysis from pyruvate. Click here to review the alkane pathway. We hypothesize that if we increase the resources required for the production of alkanes, then the cell will produce more alkanes.

Once it is determined that we have sufficient pyruvate production from our cyanobacteria (as determined by the pyruvate kinase assay), we will do lipid profiling by gas chromatography to verify the lipid produced is the substrate needed for the cell to produce alkanes. Gas chromatography takes the initial compound we wish to analyze (lipid produced from our cyanobacteria with over-expression of pyruvate kinase) and binds it to the liquid on the walls of the gas chromatography column. The lipid reacts with an added inert gas. This process yields a peak in the spectrum specific to the lipid in question. We anticipate that the lipid produced by our cyanobacteria will be the substrate for the cell to undergo the fatty-acid pathway to produce alkanes.

The next step will be to confirm that alkane production has been completed by the cell. Working with our mentor, Dr. Fenton, we will also use gas chromatography to verify the alkane produced.