Revision as of 08:37, 18 October 2020

Requirements of the Biofilm Displaying our Enzymes Improvement of Biofilm Formation Obviation of Sporulation Final Bacillus Subtilis Flow Chamber Atomic Force Microscopy Small Molecule Sorption

Requirements of the Biofilm

Bacillus subtilis

enzymes

be exported into the extracellular matrix

avoid

getting washed away

absorb the substances

prevent GMO release

biofilm into the environment

resist mechanical pressure

exposed in wastewater treatment plants

Biofilm engineering

Displaying our Degradation Enzymes in the Biofilm Matrix

The Major Biofilm Matrix Component (TasA)

The Bacillus subtilis biofilm matrix consists mainly of exopolysaccharides (EPS) and proteins. One protein essential for the structure and formation of a biofilm is the major biofilm matrix component (TasA).^[1] It polymerizes into long amyloid-like fibres which are attached to the cell wall by the TasA anchoring protein (TapA) outside of the cell.^[2] The knockout of tasA leads to a mutant that forms a weak biofilm of decreased thickness.^[3] B. subtilis secretes proteins in order to enable intercellular linkages and communication and therefore uses the Sec-dependent signal recognition particle (Sec-SRP) pathway. For proteins to be secreted via the SPR pathway, it is necessary that the proteins possess a 27 amino acids long N-terminal signal peptide, which is cleaved off during the membrane translocation. Following this scheme, TasA also possesses this N-terminal signaling peptide.^[4,^5] The Sec-SRP pathway consists of four main steps: 1) the signal peptide is recognized by a ribonucleoprotein complex, the signal recognition particle (SRP). 2) SRP targets the Sec translocase which transports the protein through the membrane. 3) during membrane translocation the signal peptide is cleaved off by the SipW peptidase leading to the release of the protein. 4) chaperones mediate the correct folding of the protein outside the cell.^[5]

A Fusion Protein of TasA with our Degradation Enzymes

We want to immobilize our degradation enzymes in the biofilm matrix, due to the improved stability and improved enzyme activity of immobilized enzymes.^[6] Furthermore, within the biofilm matrix the degradation targets are better accessible for enzymatic degradation than within the cytoplasm. Therefore, we decided to generate fusion proteins with our degradation enzymes and the protein TasA, following previous work by Huang et al..^[7]

Figure 1:
EDIT ME
The genes of the proteins for the fusion protein are linked by a linker

They showed that fusion proteins consisting of TasA and a second protein domain (e.g. mCherry, SpyTag) are successfully exported into the biofilm matrix. Even a fusion protein of TasA with the larger enzyme MHETase (63.1 kDa) was localized in the biofilm matrix of B. subtilis. Based on the research of Huang et al., we planned the fusion protein of superfolder green fluorescent protein (sfGFP) with TasA as a proof of concept. The sequence of the sfGFP gene is codon optimized for B. subtilis and fused to the C-terminus of the tasA gene with a gene fragment encoding a glycine-serin-rich linker (ARGGGGSGGGGS). The display of the TasA-sfGFP fusion protein in the biofilm matrix can be verified using fluorescence microscopy. If TasA-sfGFP is successfully expressed in the biofilm matrix, we hypothesize that analogously designed TasA fusion proteins with our targeted degradation enzymes CotA, CueO and EreB will likely succeed.

Integration of the TasA Fusion Proteins in the B. subtilis Genome

We want to ensure that only TasA fusion proteins, but no endogenous TasA, are secreted into the matrix in order to increase the number of immobilized degradation enzymes in the biofilm matrix. Therefore, we use a B. subtilis TasA knockout strain supplied by the group of Prof. Stülke (Georg-August-Universität Göttingen).^[8] Then as a proof of concept, the TasA fusion protein will be introduced in B. subtilis via plasmids (see Huang et al.). In the next step we want to integrate the TasA fusion proteins into the genome of our B. subtilis strain. For further information on the workflow and analysis of our concept, please refer to our next on Engineering Success.

Improvement of Biofilm Formation

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Quellen 9-12

Figure #: Another very nice parallelogram

Obviation of Sporulation

Bacillus subtilis is able to form endospores. During B. subtilis biofilm maturation, cells can sporulate and leave the biofilm ^[13] which could cause an escape of our genetically modified organisms into the environment. Since endospores are physiologically inactive, they do not express enzymes and thus do not contribute to micropollutant degradation. For these reasons, we aim to prevent any sporulation in the biofilm population.
The sigma factor F (σ^F) plays a critical role in the sporulation of B. subtilis by controlling several required genes ^[14] (Abbildung). The absence of σ^F renders B. subtilis unable to sporulate ^[15] , which is why we want to knockout the sigF gene in the genome of our B. subtilis.

Figure 1: The knockout of *sinR* improves biofilm formation while the knockout of *sigmaF* prevents sporulation.

Final Bacillus Subtilis

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Testing

Flowchamber

Atomic Force Microscopy

A Atomic Force Microscopy (AFM) is a probe microscope with an up to 1000-fold higher resolution than common microscopes.^[17] ^[18] By measuring the surface, it will give precise information about the topology of our biofilm. A typical AFM setup is shown in Figure 1. The imaging process works with the offset of the laser pointing at the cantilver’s back, as well as the mechanical force bending the cantilever back.
AFM is capable of different measuring modes, that are favourable in varying conditions. For a biofilm’s soft surface, the non-contact mode is preferable. Since it reduces the friction of the cantilever’s tip on the surface.^[19]
Using our 3D printed flow chamber experiments in combination with AFM data analysis, we can determine the stability of our biofilm. How we will use the flow Chamber in Combination with the AFM you can see here.

Quelle 17-19

Assay Small Molecule Sorption into the Biofilm

We want to produce our pollutant-degrading enzymes fused to one of the B. subtilis biofilm-forming proteins, the major protein component (TasA). This way it will be displayed in the matrix of the biofilm. We need to make sure that the substances are able to enter the biofilm to be converted by our displayed enzymes. Here we focused on the sorption of diclofenac because it poses the biggest issue in wastewater treatment plants. Torresi et al. recently established an assay to measure the uptake of small molecules into biofilms of various thickness on which our assay is based on.^[20]

We grow the biofilm directly on carriers used in wastewater treatment to make the experiment as realistic as possible. After the biofilm is formed on the carriers, we test the diclofenac uptake. Therefore, we incubate the carriers with different concentrations of diclofenac and take samples of both the solution and the biofilm at certain time points. The biofilm sample is resuspended in water, centrifuged and washed repeatedly. After that, the cells are lysed via sonification and the suspension is centrifuged again to clear the lysate. The supernatants of this step and the samples of the diclofenac solutions are quantified via UV after HPLC separation. If diclofenac is absorbed by the biofilm at the assayed concentrations, we will do the same with concentrations that can be found in wastewater in Germany and then analyze the taken samples via LC-MS because it is more sensitive than HPLC with UV detection.^[21]

Figure 1: The biofilm is grown on plastics carrier. This takes approximately 5 days. Afterwards, the biofilm is put in diclofenac solution and samples are taken at certain time points to analyze via HPLC.

Importantly, plastics has shown adsorption of hydrophobic substances.^[22] On that account, we perform the same assay with an empty carrier in diclofenac solution to see potential adsorption to the carrier itself.

Evaluation

We are confident that the biofilm will grow on these carriers, because the material is the same as used in the flowchamber where it grew (Verlinkung auf Flowchamber results). Furthermore, the carrier material was recommended by Prof. Dr. Lackner and these carriers are a common method in moving bed biofilm. reactors^[23] If the biofilm does not grow, we will try and use a different more porous carrier such as pumice stone or ceramics. Biofilm growth on the carrier is detectable by a mucous layer on the floating body which is visible by eye.
Diclofenac is a hydrophobic molecule which is positively charged at pH 7.4.^[24] The B. subtilis biofilm matrix is negatively charged and hydrophobic as well so diclofenac should be able to be absorbed into the biofilm.^[25] This test will be successful if the HPLC analysis shows a decrease of diclofenac even at low concentrations over time so we can test at real-life concentrations. The paper we based our assay on also tested diclofenac biofilm sorption but could not see a significant decrease of diclofenac in their bioreactor.^[20] As they used activated sludge and not a B. subtilis biofilm, we cannot directly compare results. Other reasons why this assay might not work could be wrong charge of the matrix or the size of the pores in the matrix. If this situation would occur, we could try to change the pH of the solution to consequently change the charge of the molecule of the matrix, e.g. the extracellular polymer poly-γ-glutamate. However, this approach would likely be not applicable in WWTP due to the high volume and later drain into the environment. Rather, we could change the conditions in which the biofilm is formed because that can affect the biofilm matrix and it also could be done in our proposed implementation.^[26] Furthermore, we would search for other solutions to make the biofilm matrix more receptive to diclofenac. That could be tried by overexpressing genes responsible for resorptive extracellular polymer substance synthesis.^[25]
Here we exemplary focused on diclofenac, but there are further substances whose uptake into the biofilm we could test since they are relevant for this project .

References

1. Branda, S.; Chu, F.; Kearns, D. (2006): A major protein component of the Bacillus subtilis biofilm matrix. In: Molecular microbiology 59 (4), S. 1229–1238. DOI: 10.1111/j.1365-2958.2005.05020.x. 2. Romero, D.; Aguilar, C.; Losick, R. (2010): Amyloid fibers provide structural integrity to Bacillus subtilis biofilms. In: Proceedings of the National Academy of Sciences of the United States of America 107 (5), S. 2230–2234. DOI: 10.1073/pnas.0910560107. 3. Dogsa, Iztok; Brloznik, Mojca; Stopar, David; Mandic-Mulec, Ines (2013): Exopolymer diversity and the role of levan in Bacillus subtilis biofilms. In: PloS one 8 (4), e62044. DOI: 10.1371/journal.pone.0062044. 4. Stöver, A.; Driks, A. (1999): Secretion, Localization, and Antibacterial Activity of TasA, a Bacillus subtilis Spore-Associated Protein. In: Journal of Bacteriology 181 (5), S. 1664–1672. 5. Ling, L.; Zi, R.; Wei, F. (2007): Protein secretion pathways in Bacillus subtilis: implication for optimization of heterologous protein secretion. In: Biotechnology advances 25 (1), S. 1–12. DOI: 10.1016/j.biotechadv.2006.08.002. 6. Brady, D., Jordaan, J. Advances in enzyme immobilisation. Biotechnol Lett 31, 1639 (2009) DOI: 10.1007/s10529-009-0076-4. 7. Huang, J., Liu, S., Zhang, C. et al. Programmable and printable Bacillus subtilis biofilms as engineered living materials. Nat Chem Biol 15, 34–41 (2019) DOI: 10.1038/s41589-018-0169-2. 8. Gerwig J, Kiley TB, Gunka K, Stanley-Wall N, Stülke J. The protein tyrosine kinases EpsB and PtkA differentially affect biofilm formation in Bacillus subtilis. Microbiology (Reading). 2014 Apr;160(Pt 4):682-691. DOI: 10.1099/mic.0.074971-0. 13. Kolter et al. (2013) Sticking together: building a biofilm the Bacillus subtilis way. Nat Rev Microbiol. 11(3): 157-168 14. Errington, J. Regulation of endospore formation in Bacillus subtilis. Nat Rev Microbiol 1, 117–126 (2003). 15. Overkamp W, Kuipers OP. Transcriptional Profile of Bacillus subtilis sigF-Mutant during Vegetative Growth. PLoS One. 2015;10(10):e0141553. Published 2015 Oct 27. DOI: 10.1371/journal.pone.0141553 17. Huang, Qiaoyun; Wu, Huayong; Cai, Peng; Fein, Jeremy B.; Chen, Wenli (2015): Atomic force microscopy measurements of bacterial adhesion and biofilm formation onto clay-sized particles. In: Scientific reports 5, S. 16857. DOI: 10.1038/srep16857. 18. Synthesis and Applications of Electrospun Nanofibers Micro and Nano Technologie 2019, Pages 257-281

19. Atomic Force Microscopy of Biofilms—Imaging, Interactions, and Mechanics By Sean A. James, Lydia C. Powell and Chris J. Wright 20.Torresi, E.; Polesel, F.; Bester, K. Diffusion and Sorption of Organic Micropollutants in Biofilms with Varying Thicknesses. Water Res. 2017, 123, 388–400 Doi: 10.1016/j.watres.2017.06.027 21.Abdel-Hamid, M. E. Comparative LC-MS and HPLC Analyses of Selected Antiepileptics and Beta-Blocking Drugs. Farmaco 2000, 55 (2), 136–145 Doi: 10.1016/S0014-827X(00)00006-9 22.Zhang, H.; Pap, S.; Taggart, M. A. A Review of the Potential Utilisation of Plastic Waste as Adsorbent for Removal of Hazardous Priority Contaminants from Aqueous Environments. Environmental Pollution. Elsevier Ltd March 1, 2020, p 113698 Doi: 10.1016/j.envpol.2019.113698 23.Andersson, S., Nilsson, M., Dalhammar, G. (2008). Assessment of carrier materials for biofilm formation and denitrification. Vatten, 64, 201–207. Retrieved from http://urn.kb.se/resolve?urn=urn:nbn:se:kth:diva-10154 24. National Center for Biotechnology Information (2020). PubChem Compound Summary for CID 3033, Diclofenac. Retrieved October 4, 2020 from https://pubchem.ncbi.nlm.nih.gov/compound/Diclofenac 25.Marvasi, M.; Visscher, P. T.; Casillas Martinez, L. Exopolymeric Substances (EPS) from Bacillus Subtilis: Polymers and Genes Encoding Their Synthesis. FEMS Microbiol. Lett. 2010, 313 (1), 1–9 Doi: 10.1111/j.1574-6968.2010.02085.x 26.Shukla, A.; Mehta, K.; Parmar, J. Depicting the Exemplary Knowledge of Microbial Exopolysaccharides in a Nutshell. European Polymer Journal. Elsevier Ltd October 1, 2019, pp 298–310 Doi: 10.1016/j.eurpolymj.2019.07.044

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