Given the problem with PFAS contaminated water, we strived to eliminate PFOA (one of the most widespread PFAS) from water supplies.
Since we are working on optimizing a set of dehalogenases, we need a system that can allow us to select the most efficient bacteria. Our part BBa_K4868001 is a composite part consisting of two parts:
When the dehalogenases degrade PFOA and cleave the C-F bonds, fluoride is released. This will activate the riboswitch, resulting in the expression of the green fluorescent protein. The more effective the dehalogenases are at degrading PFOA, the more fluoride will be released, and the more the cells will fluoresce. The principle of the selection system can be seen on figure 1, and the basic mechanism of a riboswitch can be seen on figure 2.
To insert the dehalogenases after the DNA construct has been assembled in a backbone, we use the highly efficient Golden Gate Cloning method. The site where the dehalogenase will be inserted is occupied by a red fluorescent protein gene, which is replaced during the Golden Gate Cloning. Colonies that do not have the dehalogenase gene inserted will fluoresce red and can therefore be easily detected.
The design we chose shaped the methods we used in the project. Here are short descriptions of what methods we used and why. Detailed descriptions of these methods can be found in the dropdown “Method Details” at the bottom of the page.
Plasmid assembly: To construct a plasmid for transformation, we used Gibson Assembly. Due to problems with synthesizing our insertion piece, we had to have it synthesized in two parts. Gibson Assembly is useful for inserting multiple fragments at once into a backbone.
Insertion of dehalogenases: The dehalogenase genes needed to be inserted into the plasmid after assembly, in an efficient manner. For this, we chose the Golden Gate Cloning technique, where we utilized the PaqCI type IIS restriction enzyme.
Mutagenesis: To create a huge library of mutants, as a means of creating better dehalogenases, we opted for untargeted mutagenesis with Error-prone PCR.
Selection of optimized enzymes: After creating an array of mutants, we needed a way to select the most efficient bacteria. Given the correlation between fluorescence and degradation efficiency, we decided to use FACS to sort the most fluorescent cells.
Protein purification: Since we wanted our final product to be purified enzymes, we used the HisCube - Ni-INDIGO His-Tag Protein Purification MINI Kit. The purification was verified with SDS-Page.
Measuring efficiency: It was essential to evaluate the efficiency and kinetics of our purified enzymes, and for this we used F-NMR and a fluoride probe, to measure the release of fluoride during the degradation.
Initially in our project, we wanted to create a strain of E. coli with an increased tolerance to fluoride. This would be beneficial in the experimental procedures generating more efficient dehalogenases, where the bacteria could be exposed to high concentrations of fluoride from the degradation process. Though we did succeed, we later learned that the fluoride tolerance would not be beneficial in our project, as described on the Engineering page.
To create this tolerant strain, we used Assisted Laboratory Evolution (ALE), where a selection pressure of increasing fluoride concentrations, and a mutagen, are applied to accelerate adaptation towards higher tolerance.
We used Gibson assembly to insert the two parts of our insertion piece into our plasmid backbone, which, before the assembly, was cut and linearized with the restriction enzymes SgrAI and HindIII.
For the Gibson assembly to be successful, we added 30 base pair overhangs to both sides of both parts of the insertion piece. The added overhangs are identical to the DNA parts where the assembly will be taking place. This way the 5' exonuclease will create single-stranded overhangs that will be complementary and seamlessly assemble our insertion piece into our plasmid backbone.
Golden Gate Cloning is a method for assembling DNA fragments. The method utilizes the IIS-restriction enzymes, where we specifically used PaqCI. Two or more DNA fragments flanked with compatible recognition sites can then be digested and seamlessly ligated. Because the product will no longer contain the original recognition site, there will be no re-digestion, driving the process towards 100% completion.
Golden gate cloning was chosen since the design would allow the red fluorescent protein to be cut out, and the DeHa enzymes to be inserted in its place. Our Golden Gate insertion site is controlled by the T7 promoter, which means that under the presence of IPTG, the colonies will either turn red or white depending on whether the cloning was successful. In this way, we also ensured that the colonies we selected for further analysis had received the DeHa, since it is not possible for the plasmid to re-ligate itself without DeHa, because of the overhangs we designed1. Figure 4 gives an overview of the RFP-dehalogenase exchange that happens in Golden Gate cloning.
Since there were several unknown factors about the enzymes, it would be difficult to make targeted modifications. This is why we are using random mutagenesis instead. Error-prone PCR was chosen to create DeHa mutant libraries.
This approach was chosen because, unlike using in vivo mutation of the DeHa gene to generate diverse isotypes, this approach prevents mutations in the host metabolism and the riboswitch-selection system. This means we can be sure that improved PFOA degradation will be caused by a more efficient dehalogenase and not be a mutation in a different gene. This is important because the enzymes were purified following the selection process and any mutations outside the DeHa sequence would not improve the PFOA degradation in vitro.
The error-prone PCR kit from Jena Bioscience was used, which included PCR components that increase the mutation frequency of the DNA polymerase by 0.6-2.0%2. These PCR components included enhanced concentrations of magnesium ions and unbalanced levels of dNTPs. Using a Taq-polymerase, which does not proofread, increased the error rate.
Performing Error-prone PCR on the DeHa sequences isolated will ensure that there are several different sequences produced which all can be transcribed and translated to different enzymes. A schematic of an error-prone PCR reaction can be seen on figure 5.
Fluorescence-activated Cell Sorting (FACS) is a type of flow cytometry, which uses the scattering of light or fluorescence activity to sort cells. An illustration of this principle can be seen in figure 6.
FACS was chosen as it is a high-throughput way to screen the DeHa libraries, which can easily contain several thousands of different enzyme variants.
After sorting the most fluorescent cells into individual wells on 96-well plates, the cells were incubated to initiate cell division. After 24 hours of incubation, the OD600 and fluorescence were measured which made it possible to select the most fluorescent bacterial lines among the variants. From the selected bacterial lines, the plasmid containing the improved dehalogenase enzyme was purified and submitted for sequencing.
After sequencing results had been assessed to make sure that the sequences differed from the original sequence and each other, the bacterial strains containing the plasmids were cultivated at a larger scale and the proteins were purified from them and tested.
The resin used in this kit consisted of cross-linked agarose beads and had a protein binding capacity of up to 100 mg/mL3. The used kit has the article no. 80101.
Sodium dodecyl-sulfate polyacrylamide gel electrophoresis (SDS-page) is a method used to separate complex mixtures of protein. The first step is the denaturation of the proteins with an anionic detergent, which also binds to the protein, giving them a negative charge proportional to the protein's molecular mass. This is followed by electrophoresis, where the porous acryl gel matrix separates the proteins according to their size. The predicted result of an SDS-page resulting from the purified dehalogenases DeHa 1, 2 4, and 5 can be seen on figure 7.
We chose to use F-NMR since fluoride has a spin. It is possible to measure how the PFOA molecules are cut by the enzyme without the enzyme interfering with the measurements (because the enzymes do not contain Fluorine). F-NMR was used to determine if and how fast the enzymes work.
Firstly, F-NMR is used to determine whether the enzyme cleaved the F-C and C-C bonds. This can be seen if the peaks in the spectra have shifted or disappeared. Afterward, F-NMR was used to study the kinetics of the enzymes, by taking an F-NMR spectra at regular intervals and comparing the spectra and see how the peaks “move around” in the spectra.
Fluorine-19 nuclear magnetic resonance spectroscopy (F-NMR) is a method typically used for structural analysis of molecules. This method takes advantage of the fact that certain nuclei have a spin. A Spin depends on the isotope of the element. When applying an external magnetic field, the nuclei will align with or against the field. Then a radio frequency is applied that makes the nuclei temporarily shift alignment. When the radio frequency is turned off, the nuclei emit energy which is detected, and results in an interpretable spectrum4. An example of such a spectrum can be seen in figure 8.
One of the final planned experiments of this project was to measure the enzymatic activity of the variant dehalogenases and compare it to the original dehalogenases, using an ion-sensitive electrode. Unfortunately, due to delivery issues, it was not possible to obtain the electrode before The Grand Jamboree. It would have been a valuable tool for determining the enzymatic activity of both the original and variant dehalogenases. An ion-sensitive electrode measures the electric potential of a solution, which results from the presence of ions. By measuring the electric potential of stock solutions with known fluoride concentrations, a reference curve could be created. With this reference curve, the electric potential of the solution can be converted to the concentration of fluoride.
In essence, the planned experiment involved creating several PFOA solutions corresponding to the number of dehalogenases to be tested. All would have the same PFOA concentration. Next, the desired enzyme would be added to its respective beaker. PFOA degradation using the dehalogenases of interest yields free fluoride ions, which would affect the electric potential of the solution. The electrode would then be used to measure the electric potential of the solutions over time, at set intervals. Using the reference curve, the data points could be converted to the fluoride concentration of the respective solutions at a given time. Thereby, the change in fluoride concentration over time could be calculated, and from this, enzymatic activity would be derived.
In conclusion, an ion-sensitive electrode would allow for the measurement of the enzymatic activity of both the original and variant dehalogenases. This would reveal whether optimization of dehalogenases using error-prone PCR is feasible.
For further information on how this experiment would have been conducted, please refer to SOP 30.
It was official. We hit a wall. The working theory was that the increased fluoride tolerance came from optimized efflux pumps. This meant that both strains could maintain a very low intracellular concentration of fluoride. To verify this proposal, both ALE1 and ALE2 were sent to whole genome sequencing. Whole genome sequencing would also reveal why ALE2, but not ALE1 showed fluorescence. In any case, both ALE strains were unfit for the selection of optimized enzymes. So, the tale of ALE ended here. Not all hope was lost, though! Other strains still responded well to fluoride under the fluorescence microscope.
For further information, please visit our Results page.
Unfortunately, the whole-genome sequencing results of ALE1 and ALE2 arrived just before the wiki-freeze, leaving too little time for analysis. The analysis will be ready for The Grand Jamboree, so stay tuned!