Results
Aims
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In this experiment, we had two aims that we wished to accomplish.
- To express psiD, psiK and psiM genes individually in E.coli, replicating their known in vivo expression (Fricke, Janis, Blei, Felix, and Hoffmeister, Dirk. “Enzymatic Synthesis of Psilocybin.” Angewandte Chemie International Edition 56.40 (2017): 12352–12355. Web.).
- To characterise the functionality and kinetics of these psi genes in vitro.
Constructing psi gene Expression Vectors
Our first step successful step in the experiment was cloning of psiD, psiK and psiM genes individually into pET28 vectors (Figure 1). It was important for us to generate stable recombinant pET28 vectors as this would enable us to transform any T7 polymerase containing E.coli cell line and induce strong expression of our proteins with an added N terminal 6xHIS tag.
After using our constructs to transform BL21 E.coli cells we started testing our cell lysates for the presence of our proteins after induction. For this, we used SDS-PAGE gel electrophoresis as our diagnostic tool. In our first series of investigations, we encountered a noticeable problem. When we attempted expressing Psi proteins they appeared highly insoluble under our expression conditions (figure 2). To improve the solubility of our protein we began revising and troubleshooting our expression conditions and enlisted assistance from the Macquarie iGEM team (Figure 3) (See more about their help here!( See more about their help here!)
Achieving soluble Psi protein expression
Insoluble expression at 22°C
With the results obtained from Macquarie and our own data we determined that it might be necessary to modify not only our expression conditions but also our system to hopefully increase the soluble expression of our proteins.
We decided to co-transform our pET28 vectors alongside an additional vector (pGro7) encoding the molecular chaperone complex groES-groEL into new BL21 cells. We believed the added chaperone and an incubation temperature around 15C after induction would reduce the stress on our cells and increase the solubility of our proteins. After generating new SDS PAGE gels of our cell lysates we observed evidence of our Psi proteins appearing relative to our uninduced controls in our soluble cell extracts.
Confirmation of Soluble Psi Proteins
We were successful in selecting and identifying two gel spots we believed to be Psi proteins. Mascot returned significant matches with PsiM and PsiK for these bands and although we were unable to identify PsiD, and in the interest of time, we were confident that it was also expressing at our new conditions based on the results for the other two proteins. Using our new expression conditions we grew large cultures of cells containing our constructs and attempted to nickel column purify our Psi proteins from cell lysates. Due to technical errors in the lab, we were only able to recover column purified fractions we believed contained PsiD and PsiK. In the interest of time we decided to test the functionality of these Psi proteins using a qualitative LC/MS in-vitro assay modelled off Frick et al (Figure 6) (Figure 7).
Did we meet our aims?
Our LC/MS data yielded exciting results! We were able to confirm catalytic activity for both PsiD and PsiK with PsiD successfully converting L-tryptophan to tryptamine and psiK converting 4 hydroxytryptamine to norbaeocystin in vitro. We noticed the presence of a hydroxylated tryptamine compound in our PsiD assay supplemented with tryptophan. Because we also observed the formation hydroxytryptamine compound in our 1mM standard of tryptamine we suspect that tryptamine may spontaneous oxidize to form this compound and therefore its presence in our in vitro assay is not the result of any conversion by endogenous E.coli proteins. Along with our peptide mass fingerprint identification, we made considerable headway in achieving our aims as outlined below.
Future Directions?
Going forward with this experiment there are several avenues we wish to explore. We would first want to confirm soluble PsiD expression using LC/MS and peptide mass fingerprint identification. Next we would work towards purifying and quantifying all psi genes once more and use LC/MS again to characterize the functionality of PsiM. We would also like to quantify the amount of Psi protein present in our purified protein fraction. This would enable us to make estimations on the amount of protein present in each cell. Following this, we could then characterize the kinetics of our proteins using HPLC LC/MS. Sampling our in vitro assay containing a known amount of protein during a time course, after the addition of respective substrates, should help us build a kinetic profile for our enzymes. This information would be highly valuable in helping model systems designed using these parts.
Aim
To take the three genes psiD, psiK and psiM from the psilocybin enzymatic pathway that we had previously expressed using the PK18 vector and clone them into our in-house PUS250 vector which has a tightly regulated cumate promoter system and a chromoprotein allowing easy selection. We built the new construct using Golden Gate assembly and validated our results by Sanger sequencing and LCMS of metabolites.
Sequencing of pUS387 plasmid
The result of our sequencing shows a large ~400 bp deletion in the psiM part of the construct. This is concerning, as the activity of PsiM must be intact for the production of Baeocystin, which appeared in our LCMS results. This deletion also appears in the sequence of both of our PUS387 constructs which were derived from separate colonies. It seems unlikely that such a large truncation would still result in a functional enzyme and that it could appear in both Golden Gate constructs when we had confirmed the sequence of the inserts was correct. However, diagnostic restriction digest of the PUS387 constructs shows a degraded band of ~500bp which corresponds to the appropriate size of a truncated PSIM protein. There is also the possibility that E. coli contains an endogenous methyltransferase that can catalyse the conversion of Norbaeocystin to Baeocystin. The ability of this protein to still be catalytically active requires further investigation.
Future Directions
Although we have demonstrated that the enzymes in the pathway are active in the construct we were unable to demonstrate the production of Psilocybin. We postulate that this is due to low levels of activity and insufficient production of Baeocystin to drive the equilibrium of the reaction towards the product. Future work will need to focus on the optimisation of the conditions for protein production. This may involve the optimisation of growing media, conditions and the use of chaperone proteins. One potential optimisation pathway could include the use of error-prone PCR and to screen for and improved protein production phenotype.
Dual Plasmid Assay
We have cloned both the PUS382 and PUS383 plasmids which contain the gene for psiH into DH5 pGro7 and performed a resting metabolism assay but are yet to receive the LCMS results. This is a key part of our experiment to recreate the entire Psilocybin synthesis pathway in a single organism and brings us closer to our aim of bulk production.
Considerations for replication of experiments
The unusual sequencing results for the construct will need to be resolved by designing primers to span the putative region of the deletion. Additionally, we need to purify the PSIM protein from our constructs and test its activity with a quantitative assay such as HPLC-MS. This will confirm whether there is a true deletion, some other mutation or an issue with our primer design and will allow us to better characterise the construct. If the deletion is confirmed we will need to rebuild the construct with the correct PSID insert and compare their activities to see if we can improve the efficiency of the construct.
Aim
This part of the project aimed to express and characterise the activity of the PsiH enzyme in vivo before putting it into our single-cell system.
Plasmid Construction
The first step was to excise the human p450 gene from the pCW plasmid and then re-ligate the plasmid back together. This was achieved, and the plasmid pUS381 was created. From there, we could clone in our wild type PsiH gene, making pUS382, and the codon optimised PsiH gene, making pUS383. The maps of these plasmids can be seen in Figure 1, and restriction digests can be seen in figure 2.
After constructing each plasmid (pUS381, pUS382 and pUS383), they were sent off for Sanger sequencing. It was confirmed that pUS381 and pUS382 were correct. However, we found out that in pUS383, there was a single nucleotide deletion at the start of the codon optimised PsiH gene. This results in a frame-shift mutation and a truncation of the protein. Unfortunately, this sequencing data only came back after we had performed all of the assays, and we did not have time to re-do them.
Protein Expression of psiH
To confirm that our protein could be expressed in E. coli, we set up cultures of cells containing the plasmids pUS381, pUS382, and pUS383. Each plasmid had two cultures – one that was induced with IPTG and one that was uninduced. The insoluble fraction from these proteins was run on an SDS PAGE gel and imaged with stain-free imaging.
The SDS PAGE gel clearly shows bands (highlighted with red boxes) that appear in the cell lysate from induced cultures containing PsiH – pUS382 and pUS383. They do not appear in the cell lysates of uninduced cells, or cells that had the pUS381 plasmid with no PsiH. These bands are therefore probably PsiH. PsiH is a 57kDA protein, but because it is a membrane-bound protein, it can appear on gels at a slightly different size. This explains why the PsiH bands on this gel appear to be approximately 50kDa.
As mentioned earlier, the pUS383 construct had a single nucleotide deletion, resulting in a frameshift mutation. This frameshift results in a truncation and brings the molecular weight of the protein down to 52kDa. It can be seen that the PsiH band in the pUS383 induced fraction is slightly lower on the gel than the band in the pUS382 fraction
Another SDS PAGE gel of the same samples was run and stained with Coomassie blue (shown in Figure 4), to be sent off Mass Spectrometry analysis of the protein. The Coomassie staining makes it harder to see the PsiH proteins. However, it does show other relevant proteins. As indicated in Figure 4, the 70kDa cytochrome p450 reductase partner protein, which is also under IPTG inducible control, can be seen in the induced cell lysates. There is also a very large band which is likely to be the 60kDa chaperone proteins, groES, that we are using to help with PsiH expression.
Despite being able to see bands on the gel, the Mass Spectrometry results were unable to identify PsiH. This does not mean that PsiH was not present - rather, it means that PsiH was not the most abundant protein in the portion of gel that was analysed.
Testing PsiH enzyme function - Indole Assay
After seeing that our PsiH proteins were being expressed we wanted to test their functionality, so we decided to do an indole assay. Many p450 monooxygenases can oxidize indole to make coloured compounds such as indigo. E. coli cells contain endogenous indole, so when grown in the right conditions, cells containing functional p450 monooxygenases can turn blue. This assay takes around 5 days and has many complicated components. We used a positive control, the pCW plasmid containing a human p450 monooxygenase which is known to turn indole to indigo so that we could tell if we had performed the assay correctly. We also used a negative control, the pUS381 plasmid that had no p450 monooxygenase. For each plasmid type, we grew up two cultures, and then induced one and left the other uninduced so we could compare the colours. The results of this experiment show that the induced culture of cells containing pCW turned blue, but none of the other induced cultures changed colour (as shown in figure 5). We did not expect to see a colour change in the pUS381 culture, as it contains no p450 enzyme. Retrospectively, it was also impossible that there would have been a colour change in the pUS383 culture either, because of the frameshift mutation in the codon optimised PsiH in this plasmid. Therefore, this assay only gives us information about the wt PsiH gene in our pUS382 plasmids
This assay could reveal one of two things about that wt PsiH gene - either it was expressing but was not functional, or was functional but could not oxidise indole or is doing so in such a small amount that it was impossible to see. In order to determine which of these conclusions is correct, we needed to perform another assay.
Testing PsiH enzyme function - Tryptamine assay
This assay was performed to test the ability of PsiH to catalyse the reaction that it performs in the psilocybin biosynthesis pathway, the oxidation of tryptamine to 4-hydroxytryptamine.
The LCMS results were difficult to analyse. The reason for this was that a substance of the same molecular mass and composition as 4-hydroxytryptamine was found in our ‘pure’ tryptamine standard. We also saw this compound in our negative control (cultures with pUS381) and in our culture with pUS383, which we now know has a mutated psiH. However, we did not see any of this compound in our culture expressing the correct PsiH. This compound may have been 4-hydroxytryptamine, but may also have been 5 or 6-hyroxytryptamine - LCMS is unable to distinguish between them. These results are unexpected and contrary. Firstly, they show that our PsiH gene was probably non-functional. Secondly, they may show that tryptamine can auto-oxidise to some compound that is the same or very similar to 4-hydroxytryptamine. This can potentially confuse any attempted analysis of PsiH function with this assay.
Conclusions
Ultimately, while we were able to induce E. coli cells to express PsiH, it was not found to be functional on either indole or its substrate, tryptamine. This result is not surprising, as we thought that PsiH would have to be codon optimised or harmonised to work in E. coli. Unfortunately, we were unable to test the codon optimised PsiH function in E. coli due to a frameshift mutation in the gene that drastically changed the coding sequence.
Future directions
Future directions of PsiH should be focused on further adapting the sequence of the gene for better expression in E. coli. This could be achieved by modifying the N-terminal of the gene and trying different harmonisation and optimisation methods. Additionally, different p450 reductase partner enzymes could be tested along with PsiH, such as fungal variants.
Aim
Express PsiD, PsiK, PsiM and PsiH in DH5-alpha and assess enzyme function using LC/MS.
We were able to successfully transform our chassis with our two plasmids, pUS387 and pUS382. With this transformation, we now had our first iteration of Magi.coli! - An organism with all wild type psi genes. This was as far as we got with our two plasmid system. We set up metabolic resting cell assays using cultures containing these constructs, however we have yet to gather LC/MS data for this assay.
While we have not achieved our ultimate aim with this experiment so far, we are happy with our progress :D.
Future directions
The most immediate direction we can take with this experiment would be performing LC/MS on our resting cell assays in the presence of excess tryptophan and determine how functional the system is.
Aim
The aim of this experiment was to investigate and compare the growth of our chassis organism in two separate systems:
- Fermenter: The culture was grown in batch mode using a BIOSTAT A fermenter (Sartorius). The fermenter had two six-bladed Rushton impellers, a stirrer speed of 750 rpm was used, the airflow rate was 1 vvm (1.5 L/min). A 1.5 L working volume was used, foaming was controlled via the addition of a 2% (v/v) solution of Antifoam A (Sigma) using an automated foam probe. The temperature was maintained at 37 ℃. Temperature and pH were logged using the in-built data-logging software at a rate of one sample per minute (Figure 1).
- Lab culture: The culture was grown at 37oC with shaking at 200rpm in a 2L conical flask. A 1.5L culture volume was used.
The results of this exercise demonstrated that the fermentation system is vastly superior in cultivating the growth of our chassis in our media of choice. The number of cells per litre of culture grown was 7.43 times higher in the fermenter than the lab culture over 7 hours. Growth in the fermented culture was so effective the culture had exhausted its nutrient supply by hour 6 resulting in a decline steady decrease in cell density.
Going forward we would like to optimize our Magi.coli for expression at these conditions to take advantage of this stark difference in growth.
Aim
The aim of this experiment was to determine which type of codon harmonisation/ optimisation (rank-order method, absolute frequency method, relative frequency method and IDT codon optimisation) would improve the expression of the VVD protein compared to the wild-type codon usage. CH1 was harmonised by rank order, CH2 by nearest frequency, CH3 by relative proportion and CH4 used the IPT codon optimisation tool available here. The harmonisation method descriptions can be found under the documentation for software. The results of this experiment would then be used to codon harmonise our psi genes to improve their expression.
Considerations for Replication
Through this experiment, we have concluded that codon harmonisation and optimisation may not be the most efficient method for improving the activity of these fluorescent proteins. We had significantly more success with our error-prone PCR improvement (see Error-Prone PCR of Vivid). Codon harmonisation and optimisation are essential for other expression applications in particular where the speed of translation may need to be limited to ensure appropriate protein folding.
Future Directions
We experienced some difficulty in maintaining the stability of the pk18 VIVID constructs in TOP10 cells. This may be since pk18 is a high copy number plasmid with constitutive expression and may have caused stress to the TOP10 cells. Stability may be improved using an Inducible rather than constitutive vector.
Literally 3 months of painful work with failures left and right...
Aim
The aim of this experiment was to use error-prone PCR to generate a more fluorescence version of the weakly fluorescent Vivid protein from the fungi, Neurospora crassa.
More on the background of this partError prone PCR
Error prone PCR was performed on the weakly fluorescent codon optimised vivid gene. The PCR products, when ligated in plasmids and transformed into E. coli, yielded 12 colonies that were brighter than the rest (Figure 1).
The sequencing results of the vivid genes from these bright colonies revealed that there was a common mutation in the majority of these genes (see Figure 2). This mutation modified the methionine at residue 130 to either isoleucine (found in 5 of the mutants), a threonine (found in three of the mutants), or a leucine residue (found in one of the mutants).
When a G-Block of the vivid gene containing a Methionine to Isoleucine change at residue 130 was cloned into E. coli and compared to vivid genes without the mutation, it was seen to be much brighter (Figure 3). This confirmed that it was the mutation away from methionine at residue 130 that improved the fluorescence of the protein.
A fluorescence assay was performed that compared the original codon harmonised fluorescence Vivid, the wild type fluorescent Vivid, an empty plasmid, and the new brighter Met130Ile Vivid protein (see Figure 4). This shows the extent to which the single amino acid mutation increased the fluorescence of the protein.
Lastly, the excitation and emission spectra of the new Met130I Vivid protein was measured (figure 5). This spectrum is remarkably similar to the spectra of CFP, meaning that our fluoroprotein can be used as a substitute for this fluoroprotein.Conclusion
Error prone PCR was used to create a more fluorescent version of the fungal protein, Vivid.
Future directions
Future work should focus on characterising the protein so that its usefulness can be compared to other fluoroproteins can be established.