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Cells contain a finite set of resources that must be distributed across many processes to ensure survival. Among them, the largest proportion of cellular resources is dedicated to protein translation. Synthetic biology often exploits these resources in executing orthogonal genetic circuits, yet the burden this places on the cell is rarely considered. Here, we develop a minimal model of ribosome allocation dynamics capturing the demands on translation when expressing a synthetic construct together with endogenous genes required for the maintenance of cell physiology. Critically, it contains three key variables related to design parameters of the synthetic construct covering transcript abundance, translation initiation rate, and elongation time. We show that model-predicted changes in ribosome allocation closely match experimental shifts in synthetic protein expression rate and cellular growth. Intriguingly, the model is also able to accurately infer transcript levels and translation times after further exposure to additional ambient stress. Our results demonstrate that a simple model of resource allocation faithfully captures the redistribution of protein synthesis resources when faced with the burden of synthetic gene expression and environmental stress. The tractable nature of the model makes it a versatile tool for exploring the guiding principles of efficient heterologous expression and the indirect interactions that can arise between synthetic circuits and their host chassis because of competition for shared translational resources.
Synthetische Transkriptionsfaktoren bestehen wie natürliche Transkriptionsfaktoren aus einer DNA-Bindedomäne, die sich spezifisch an die Bindestellensequenz vor dem Ziel-Gen anlagert, und einer Aktivierungsdomäne, die die Transkriptionsmaschinerie rekrutiert, sodass das Zielgen exprimiert wird. Der Unterschied zu den natürlichen Transkriptionsfaktoren ist, sowohl dass die DNA-Bindedomäne als auch die Aktivierungsdomäne wirtsfremd sein können und dadurch künstliche Stoffwechselwege im Wirt, größtenteils chemisch, induziert werden können. Optogenetische synthetische Transkriptionsfaktoren, die hier entwickelt wurden, gehen einen Schritt weiter. Dabei ist die DNA-Bindedomäne nicht mehr an die Aktivierungsdomäne, sondern mit dem Blaulicht-Photorezeptor CRY2 gekoppelt. Die Aktivierungsdomäne wurde mit dem Interaktionspartner CIB1 fusioniert. Unter Blaulichtbestrahlung dimerisieren CRY2 und CIB1 und damit einhergehend die beiden Domänen, sodass ein funktionsfähiger Transkriptionsfaktor entsteht. Dieses System wurde in die Saccharomyces cerevisiae genomisch integriert. Verifiziert wurde das konstruierte System mit Hilfe des Reporters yEGFP, welcher durchflusszytometrisch detektiert werden konnte. Es konnte gezeigt werden, dass die yEGFP Expression variabel gestaltet werden kann, indem unterschiedlich lange Blaulichtimpulse ausgesendet wurden, die DNA-Bindedomäne, die Aktivierungsdomäne oder die Anzahl der Bindestellen, an dem sich die DNA-Bindedomäne anlagert, verändert wurden. Um das System für industrielle Anwendungen attraktiv zu gestalten, wurde das System vom Deepwell-Maßstab auf Photobioreaktor-Maßstab hochskaliert. Außerdem erwies sich das Blaulichtsystem sowohl im Laborstamm YPH500 als auch im industriell oft verwendeten Hefestamm CEN.PK als funktional. Des Weiteren konnte ein industrierelevante Protein ebenso mit Hilfe des verifizierten Systems exprimiert werden. Schlussendlich konnte in dieser Arbeit das etablierte Blaulicht-System erfolgreich mit einem Rotlichtsystem kombiniert werden, was zuvor noch nicht beschrieben wurde.
One-carbon (C1) compounds are attractive microbial feedstocks as they can be efficiently produced from widely available resources. Formate, in particular, represents a promising growth substrate, as it can be generated from electrochemical reduction of CO2 and fed to microorganisms in a soluble form. We previously identified the synthetic reductive glycine pathway as the most efficient route for aerobic growth on formate. We further demonstrated pathway activity in Escherichia coli after expression of both native and foreign genes. Here, we explore whether the reductive glycine pathway could be established in a model microorganism using only native enzymes. We used the yeast Saccharomyces cerevisiae as host and show that overexpression of only endogenous enzymes enables glycine biosynthesis from formate and CO2 in a strain that is otherwise auxotrophic for glycine. We find the pathway to be highly active in this host, where 0.125 mM formate is sufficient to support growth. Notably, the formate-dependent growth rate of the engineered S. cerevisiae strain remained roughly constant over a very wide range of formate concentrations, 1-500 mM, indicating both high affinity for formate use and high tolerance toward elevated concentration of this C1 feedstock. Our results, as well the availability of endogenous NAD-dependent formate dehydrogenase, indicate that yeast might be an especially suitable host for engineering growth on formate.
Climate change, driven by increasing atmospheric levels of carbon dioxide (CO2), presents a significant societal challenge for the 21st century. Biotechnological approaches for microbial production of commodity chemicals and fuels offer possible solutions to re-fix CO2 from the atmosphere, thereby mitigating carbon emissions and contributing to a sustainable carbon-economy in the future. Biological CO2 fixation is also at the heart of agricultural productivity, where photosynthesis and the Calvin-Benson-Bassham cycle present promising biotechnological targets for crop improvement.
Synthetic biology allows testing metabolic solutions not known to exist in nature, which may exceed their natural counterparts in terms of efficiency. In this thesis, I explore the design of such new-to-nature metabolic pathways for biological CO2 utilization and their implementation in living cells (in vivo).
In the first chapter, I describe the development of a metabolic pathway that enables intracellular conversion of CO2 to formate, giving access to highly efficient carbon fixation routes. In nature, CO2-reduction remains restricted to anaerobic organisms and low redox potentials. Here, we introduce the “CORE cycle”, a synthetic metabolic pathway that converts CO2 to formate under fully aerobic conditions and ambient CO2 levels, using only NADPH as a reductant. We leverage this synthetic, ATP-energized pathway to overcome the thermodynamic and kinetic barriers associated with CO2-reduction. Applying rational metabolic engineering and adaptive evolution, this work demonstrates that Escherichia coli can utilize ambient CO2 as the sole source of one-carbon units and serine, achieving a first step towards novel modes of synthetic autotrophy. We further apply computational modeling to showcase the potential of the CORE cycle as a photorespiratory bypass for enhancing photosynthesis.
In the second chapter, I describe the development of the “LCM module”, a novel metabolic route for CO2-incorporating conversion of acetyl-CoA to pyruvate. This route relies on the newly uncovered, promiscuous activity of an adenosylcobalamin (B12)-dependent enzyme, which we significantly optimize through targeted hypermutation and in vivo selection strategies. The LCM module provides a shorter and more efficient pathway for acetyl-CoA assimilation compared to natural routes, offering novel opportunities for synthetic CO2 fixation.
Overall, through theoretical pathway analysis, enzyme bioprospecting, and modular metabolic engineering in E. coli, this thesis expands the solution space for biological CO2 fixation.
With Saccharomyces cerevisiae being a commonly used host organism for synthetic biology and biotechnology approaches, the work presented here aims at the development of novel tools to improve and facilitate pathway engineering and heterologous protein production in yeast. Initially, the multi-part assembly strategy AssemblX was established, which allows the fast, user-friendly and highly efficient construction of up to 25 units, e.g. genes, into a single DNA construct. To speed up complex assembly projects, starting from sub-gene fragments and resulting in mini-chromosome sized constructs, AssemblX follows a level-based approach: Level 0 stands for the assembly of genes from multiple sub-gene fragments; Level 1 for the combination of up to five Level 0 units into one Level 1 module; Level 2 for linkages of up to five Level 1 modules into one Level 2 module. This way, all Level 0 and subsequently all Level 1 assemblies can be carried out simultaneously. Individually planned, overlap-based Level 0 assemblies enable scar-free and sequence-independent assemblies of transcriptional units, without limitations in fragment number, size or content. Level 1 and Level 2 assemblies, which are carried out via predefined, computationally optimized homology regions, follow a standardized, highly efficient and PCR-free scheme. AssemblX follows a virtually sequence-independent scheme with no need for time-consuming domestication of assembly parts. To minimize the risk of human error and to facilitate the planning of assembly projects, especially for individually designed Level 0 constructs, the whole AssemblX process is accompanied by a user-friendly webtool. This webtool provides the user with an easy-to-use operating surface and returns a bench-protocol including all cloning steps. The efficiency of the assembly process is further boosted through the implementation of different features, e.g. ccdB counter selection and marker switching/reconstitution. Due to the design of homology regions and vector backbones the user can flexibly choose between various overlap-based cloning methods, enabling cost-efficient assemblies which can be carried out either in E. coli or yeast. Protein production in yeast is additionally supported by a characterized library of 40 constitutive promoters, fully integrated into the AssemblX toolbox. This provides the user with a starting point for protein balancing and pathway engineering. Furthermore, the final assembly cassette can be subcloned into any vector, giving the user the flexibility to transfer the individual construct into any host organism different from yeast.
As successful production of heterologous compounds generally requires a precise adjustment of protein levels or even manipulation of the host genome to e.g. inhibit unwanted feedback regulations, the optogenetic transcriptional regulation tool PhiReX was designed. In recent years, light induction was reported to enable easy, reversible, fast, non-toxic and nearly gratuitous regulation, thereby providing manifold advantages compared to conventional chemical inducers. The optogenetic interface established in this study is based on the photoreceptor PhyB and its interacting protein PIF3. Both proteins, derived from Arabidopsis thaliana, dimerize in a red/far-red light-responsive manner. This interaction depends on a chromophore, naturally not available in yeast. By fusing split proteins to both components of the optical dimerizer, active enzymes can be reconstituted in a light-dependent manner. For the construction of the red/far-red light sensing gene expression system PhiReX, a customizable synTALE-DNA binding domain was fused to PhyB, and a VP64 activation domain to PIF3. The synTALE-based transcription factor allows programmable targeting of any desired promoter region. The first, plasmid-based PhiReX version mediates chromophore- and light-dependent expression of the reporter gene, but required further optimization regarding its robustness, basal expression and maximum output. This was achieved by genome-integration of the optical regulator pair, by cloning the reporter cassette on a high-copy plasmid and by additional molecular modifications of the fusion proteins regarding their cellular localization. In combination, this results in a robust and efficient activation of cells over an incubation time of at least 48 h. Finally, to boost the potential of PhiReX for biotechnological applications, yeast was engineered to produce the chromophore. This overcomes the need to supply the expensive and photo-labile compound exogenously. The expression output mediated through PhiReX is comparable to the strong constitutive yeast TDH3 promoter and - in the experiments described here - clearly exceeds the commonly used galactose inducible GAL1 promoter.
The fast-developing field of synthetic biology enables the construction of complete synthetic genomes. The upcoming Synthetic Yeast Sc2.0 Project is currently underway to redesign and synthesize the S. cerevisiae genome. As a prerequisite for the so-called “SCRaMbLE” system, all Sc2.0 chromosomes incorporate symmetrical target sites for Cre recombinase (loxPsym sites), enabling rearrangement of the yeast genome after induction of Cre with the toxic hormonal substance beta-estradiol. To overcome the safety concern linked to the use of beta-estradiol, a red light-inducible Cre recombinase, dubbed L-SCRaMbLE, was established in this study. L-SCRaMbLE was demonstrated to allow a time- and chromophore-dependent recombination with reliable off-states when applied to a plasmid containing four genes of the beta-carotene pathway, each flanked with loxPsym sites. When directly compared to the original induction system, L-SCRaMbLE generates a larger variety of recombination events and lower basal activity. In conclusion, L-SCRaMbLE provides a promising and powerful tool for genome rearrangement.
The three tools developed in this study provide so far unmatched possibilities to tackle complex synthetic biology projects in yeast by addressing three different stages: fast and reliable biosynthetic pathway assembly; highly specific, orthogonal gene regulation; and tightly controlled synthetic evolution of loxPsym-containing DNA constructs.
Eukaryotic cells can be regarded as complex microreactors capable of performing various biochemical reactions in parallel which are necessary to sustain life. An essential prerequisite for these complex metabolic reactions to occur is the evolution of lipid membrane-bound organelles enabling compartmental- ization of reactions and biomolecules. This allows for a spatiotemporal control over the metabolic reactions within the cellular system. Intracellular organi- zation arising due to compartmentalization is a key feature of all living cells and has inspired synthetic biologists to engineer such systems with bottom-up approaches.
Artificial cells provide an ideal platform to isolate and study specific re- actions without the interference from the complex network of biomolecules present in biological cells. To mimic the hierarchical architecture of eukaryotic cells, multi-compartment assemblies with nested liposomal structures also re- ferred to as multi-vesicular vesicles (MVVs) have been widely adopted. Most of the previously reported multi-compartment systems adopt bulk method- ologies which suffer from low yield and poor control over size. Microfluidic strategies help circumvent these issues and facilitate a high-throughput and robust technique to assemble MVVs of uniform size distribution.
In this thesis, firstly, the bulk methodologies are explored to build MVVs and implement a synthetic signalling cascade. Next, a polydimethylsiloxane (PDMS)-based microfluidic platform is introduced to build MVVs and the significance of PEGylated lipids for the successful encapsulation of inner com- partments to generate stable multi-compartment systems is highlighted.
Next, a novel two-inlet channel PDMS-based microfluidic device to create MVVs encompassing a three-step enzymatic reaction cascade is presented. A directed reaction pathway comprising of the enzymes α-glucosidase (α-Glc), glucose oxidase (GOx), and horseradish peroxidase (HRP) spanning across three compartments via reconstitution of size-selective membrane proteins is described. Furthermore, owing to the monodispersity of our MVVs due to microfluidic strategies, this platform is employed to study the effect of com- partmentalization on reaction kinetics.
Further integration of cell-free expression module into the MVVs would allow for gene-mediated signal transduction within artificial eukaryotic cells. Therefore, the chemically inducible cell-free expression of a membrane protein alpha-hemolysin and its further reconstitution into liposomes is carried out.
In conclusion, the present thesis aims to build artificial eukaryotic cells to achieve size-selective chemical communication that also show potential for applications as micro reactors and as vehicles for drug delivery.
Rapid progress of experimental biology has provided a huge flow of quantitative data, which can be analyzed and understood only through the application of advanced techniques recently developed in theoretical sciences. On the other hand, synthetic biology enabled us to engineer biological models with reduced complexity. In this review we discuss that a multidisciplinary approach between this sciences can lead to deeper understanding of the underlying mechanisms behind complex processes in biology. Following the mini symposia "Noise and oscillations in biological systems" on Physcon 2011 we have collected different research examples from theoretical modeling, experimental and synthetic biology.
Microviridins are a prominent family of ribosomally synthesized and posttranslationally modified peptides (RiPPs) featuring characteristic lactone and lactam rings. Their unusual cage-like architecture renders them highly potent serine protease inhibitors of which individual variants specifically inhibit different types of proteases of pharmacological interest.
While posttranslational modifications are key for the stability and bioactivity of RiPPs, additional attractive properties can be introduced by functional tags.
To date - although highly desirable - no method has been reported to incorporate functional tags in microviridin scaffolds or the overarching class of graspetides.
In this study, a chemoenzymatic in vitro platform is used to introduce functional tags in various microviridin variants yielding biotinylated, dansylated or propargylated congeners.
This straightforward approach paves the way for customized protease inhibitors with built-in functionalities that can help to unravel the still elusive ecological roles and targets of this remarkable class of compounds and to foster applications based on protease inhibition.
Overcoming natural biomass limitations in gram-negative bacteria through synthetic carbon fixation
(2024)
The carbon demands of an ever-increasing human population and the concomitant rise in net carbon emissions requires CO2 sequestering approaches for production of carbon-containing molecules. Microbial production of carbon-containing products from plant-based sugars could replace current fossil-based production. However, this form of sugar-based microbial production directly competes with human food supply and natural ecosystems. Instead, one-carbon feedstocks derived from CO2 and renewable energy were proposed as an alternative. The one carbon molecule formate is a stable, readily soluble and safe-to-store energetic mediator that can be electrochemically generated from CO2 and (excess off-peak) renewable electricity. Formate-based microbial production could represent a promising approach for a circular carbon economy. However, easy-to-engineer and efficient formate-utilizing microbes are lacking. Multiple synthetic metabolic pathways were designed for better-than-nature carbon fixation. Among them, the reductive glycine pathway was proposed as the most efficient pathway for aerobic formate assimilation. While some of these pathways have been successfully engineered in microbial hosts, these synthetic strains did so far not exceed the performance of natural strains. In this work, I engineered and optimized two different synthetic formate assimilation pathways in gram-negative bacteria to exceed the limits of a natural carbon fixation pathway, the Calvin cycle.
The first chapter solidified Cupriavidus necator as a promising formatotrophic host to produce value-added chemicals. The formate tolerance of C. necator was assessed and a production pathway for crotonate established in a modularized fashion. Last, bioprocess optimization was leveraged to produce crotonate from formate at a titer of 148 mg/L.
In the second chapter, I chromosomally integrated and optimized the synthetic reductive glycine pathway in C. necator using a transposon-mediated selection approach. The insertion methodology allowed selection for condition-specific tailored pathway expression as improved pathway performance led to better growth. I then showed my engineered strains to exceed the biomass yields of the Calvin cycle utilizing wildtype C. necator on formate. This demonstrated for the first time the superiority of a synthetic formate assimilation pathway and by extension of synthetic carbon fixation efforts as a whole.
In chapter 3, I engineered a segment of a synthetic carbon fixation cycle in Escherichia coli. The GED cycle was proposed as a Calvin cycle alternative that does not perform a wasteful oxygenation reaction and is more energy efficient. The pathways simple architecture and reasonable driving force made it a promising candidate for enhanced carbon fixation. I created a deletion strain that coupled growth to carboxylation via the GED pathway segment. The CO2 dependence of the engineered strain and 13C-tracer analysis confirmed operation of the pathway in vivo.
In the final chapter, I present my efforts of implementing the GED cycle also in C. necator, which might be a better-suited host, as it is accustomed to formatotrophic and hydrogenotrophic growth. To provide the carboxylation substrate in vivo, I engineered C. necator to utilize xylose as carbon source and created a selection strain for carboxylase activity. I verify activity of the key enzyme, the carboxylase, in the decarboxylative direction. Although CO2-dependent growth of the strain was not obtained, I showed that all enzymes required for operation of the GED cycle are active in vivo in C. necator.
I then evaluate my success with engineering a linear and cyclical one-carbon fixation pathway in two different microbial hosts. The linear reductive glycine pathway presents itself as a much simpler metabolic solution for formate dependent growth over the sophisticated establishment of hard-to-balance carbon fixation cycles. Last, I highlight advantages and disadvantages of C. necator as an upcoming microbial benchmark organism for synthetic metabolism efforts and give and outlook on its potential for the future of C1-based manufacturing.
Plant X-tender
(2018)
Cloning multiple DNA fragments for delivery of several genes of interest into the plant genome is one of the main technological challenges in plant synthetic biology. Despite several modular assembly methods developed in recent years, the plant biotechnology community has not widely adopted them yet, probably due to the lack of appropriate vectors and software tools. Here we present Plant X-tender, an extension of the highly efficient, scarfree and sequence-independent multigene assembly strategy AssemblX,based on overlapdepended cloning methods and rare-cutting restriction enzymes. Plant X-tender consists of a set of plant expression vectors and the protocols for most efficient cloning into the novel vector set needed for plant expression and thus introduces advantages of AssemblX into plant synthetic biology. The novel vector set covers different backbones and selection markers to allow full design flexibility. We have included ccdB counterselection, thereby allowing the transfer of multigene constructs into the novel vector set in a straightforward and highly efficient way. Vectors are available as empty backbones and are fully flexible regarding the orientation of expression cassettes and addition of linkers between them, if required. We optimised the assembly and subcloning protocol by testing different scar-less assembly approaches: the noncommercial SLiCE and TAR methods and the commercial Gibson assembly and NEBuilder HiFi DNA assembly kits. Plant X-tender was applicable even in combination with low efficient homemade chemically competent or electrocompetent Escherichia coli. We have further validated the developed procedure for plant protein expression by cloning two cassettes into the newly developed vectors and subsequently transferred them to Nicotiana benthamiana in a transient expression setup. Thereby we show that multigene constructs can be delivered into plant cells in a streamlined and highly efficient way. Our results will support faster introduction of synthetic biology into plant science.