Development and application of a highly efficient CRISPR-Cas9 system for genome engineering in Bacillus megaterium

CRISPR-Cas9-mediated barcode insertion into Bacillus thuringiensis for surrogate tracking

The use of surrogate organisms can enable researchers to safely conduct research on pathogens and in a broader set of conditions. Being able to differentiate between the surrogates used in the experiments and background contamination as well as between different experiments will further improve research efforts. One effective approach is to introduce unique genetic barcodes into the surrogate genome and track their presence using the quantitative polymerase chain reaction (qPCR). In this report, we utilized the CRISPR-Cas9 methodology, which employs a single plasmid and a transformation step to insert five distinct barcodes into Bacillus thuringiensis, a well-established surrogate for Bacillus anthracis when Risk Group 1 organisms are needed. We subsequently developed qPCR assays for barcode detection and successfully demonstrated the stability of the barcodes within the genome through five cycles of sporulation and germination. Additionally, we conducted whole-genome sequencing on these modified strains and analyzed 187 potential Cas9 off-target sites. We found no correlation between the mutations observed in the engineered strains and the predicted off-target sites, suggesting this genome engineering strategy did not directly result in off-target mutations in the genome. This simple approach has the potential to streamline the creation of barcoded B. thuringiensis strains for use in future studies on surrogate genomes.

IMPORTANCE

The use of Bacillus anthracis as a biothreat agent poses significant challenges for public health and national security. Bacillus anthracis surrogates, like Bacillus thuringiensis, are invaluable tools for safely understanding Bacillus anthracis properties without the safety concerns that would arise from using a virulent strain of Bacillus anthracis. We report a simple method for barcode insertion into Bacillus thuringiensis using the CRISPR-Cas9 methodology and subsequent tracking by quantitative polymerase chain reaction (qPCR). Moreover, whole-genome sequencing data and CRISPR-Cas9 off-target analyses in Bacillus thuringiensis suggest that this gene-editing method did not directly cause unwanted mutations in the genome. This study should assist in the facile development of barcoded Bacillus thuringiensis surrogate strains, among other biotechnological applications in Bacillus species.

Effects of down-regulation of ackA expression by CRISPR-dCpf1 on succinic acid production in Actinobacillus succinogenes

Succinic acid (SA), a key intermediate in the cellular tricarboxylic acid cycle (TCA), is a 4-carbon dicarboxylic acid of great industrial value. Actinobacillus succinogenes can ferment various carbon sources and accumulate relatively high concentrations of SA, but few reliable genetic engineering tools exist for A. succinogenes and this has hindered strain improvement to increase SA production for industrial application. Two different repressors, endonuclease-deactivated Cas9 (dCas9) from Streptococcus pyogenes and Cpf1 (dCpf1) from Francisella tularensis, were applied to construct a CRISPRi system in A. succinogenes. Codon-optimized Cas9 and native Cpf1 were successfully expressed in A. succinogenes, and the corresponding sgRNA and crRNA expression elements, promoted by the fumarate reductase promoter, frd, were introduced into the CRISPRi plasmid. The highest repression of the ackA gene (encoding acetate kinase) and thereby acetic acid production (~ eightfold) was achieved by the dCpf1-based CRISPRi system, in which the mutation site, E1006A acted at the start of the coding region of ackA, the gene which regulates acetic acid biosynthesis. Compared with the ackA gene knockout mutant, cell growth was moderately improved and SA production increased by 6.3%. Further, the SA titer and productivity in a 3 L fermenter reached 57.06 g/L and 1.87 g/L/h, and there was less acetic acid production. A dCpf1-based CRISPRi-mediated gene repression system was successfully established for the first time, providing a simple and effective tool for studying functional genomics in A. succinogenes and optimizing SA production.

Versatile tools of synthetic biology applied to drug discovery and production

Although synthetic biology is an emerging research field, which has come to prominence within the last decade, it already has many practical applications. Its applications cover the areas of pharmaceutical biotechnology and drug discovery, bringing essential novel methods and strategies such as metabolic engineering, reprogramming the cell fate, drug production in genetically modified organisms, molecular glues, functional nucleic acids and genome editing. This review discusses the main avenues for synthetic biology application in pharmaceutical biotechnology. The authors believe that synthetic biology will reshape drug development and drug production to a similar extent as the advances in organic chemical synthesis in the 20th century. Therefore, synthetic biology already plays an essential role in pharmaceutical, biotechnology, which is the main focus of this review.

Development of a universal antibiotic resistance screening reporter for improving efficiency of cytosine and adenine base-editing

Base editing has emerged as a revolutionary technology for single nucleotide modifications. The cytosine and adenine base editors (CBEs and ABEs) have demonstrated great potential in clinical and fundamental research. However, screening and isolating target-edited cells remains challenging. In the current study, we developed a universal Adenine and Cytosine Base-Editing Antibiotic Resistance Screening Reporter (ACBE-ARSR) for improving the editing efficiency. To develop the reporter, the CBE-ARSR was first constructed and shown to be capable of enriching cells for those that had undergone CBE editing activity. Then, the ACBE-ARSR was constructed and was further validated in the editing assays by four different CBEs and two versions of ABE at several different genomic loci. Our results demonstrated that ACBE-ARSR, compared to the reporter of transfection (RoT) screening strategy, improved the editing efficiency of CBE and ABE by 4.6- and 1.9-fold on average, respectively. We found the highest CBE and ABE editing efficiencies as enriched by ACBE-ARSR reached 90% and 88.7%. Moreover, we also demonstrated ACBE-ARSR could be employed for enhancing simultaneous multiplexed genome editing. In conclusion, both CBE and ABE activity can be improved significantly using our novel ACBE-ARSR screening strategy, which we believe will facilitate the development of base editors and their application in biomedical and fundamental research studies.

Development of an efficient iterative genome editing method in Bacillus subtilis using the CRISPR-AsCpf1 system

Bacillus subtilis is a useful chassis in the fields of synthetic biology and metabolic engineering for chemical production. Here, we constructed CRISPR-AsCpf1-based expression plasmids with the temperature-sensitive replicon for iterative genome editing in B. subtilis. This method allowed gene insertion and large genomic deletion with an editing efficiency of up 80%-100% and rapid plasmid curing to facilitate the iterative genome editing in B. subtilis 168. Using the customized CRISPR-AsCpf1 system, we successfully and efficiently implemented the related gene editing in B. subtilis 168 for hyaluronic acid (HA) biosynthesis, HA synthase gene (hasA) insertion, UDP-glucose-dehydrogenase gene (tuaD) insertion, and eps gene cluster (epsA-O) deletion. The heterologous production of HA was realized by the engineered strain with a yield of 1.39 g/L. These results support the finding that the CRISPR-AsCpf1 system is highly efficient in bacteria genome editing and provide valuable guidance and essential references for genome engineering in B. subtilis using the CRISPR-AsCpf1 system.

Development and application of a fast and efficient CRISPR-based genetic toolkit in Bacillus amyloliquefaciens LB1ba02

Background

Bacillus amyloliquefaciens is generally recognized as food safe (GRAS) microbial host and important enzyme-producing strain in the industry. B.amyloliquefaciens LB1ba02 is a production strain suitable for secreting mesophilic α-amylase in the industry. Nevertheless, due to the low transformation efficiency and restriction-modification system, the development of its CRISPR tool lags far behind other species and strains from the genus Bacillus. This work was undertaken to develop a fast and efficient gene-editing tool in B.amyloliquefaciens LB1ba02.

Results

In this study, we fused the nuclease-deficient mutant Cas9n (D10A) of Cas9 with activation-induced cytidine deaminase (AID) and developed a fast and efficient base editing system for the first time in B. amyloliquefaciens LB1ba02. The system was verified by inactivating the pyrF gene coding orotidine 5'-phosphate decarboxylase and the mutant could grow normally on M9 medium supplemented with 5-fluoroorotic acid (5-FOA) and uridine (U). Our base editing system has a 6nt editing window consisting of an all-in-one temperature-sensitive plasmid that facilitates multiple rounds of genome engineering in B. amyloliquefaciens LB1ba02. The total editing efficiency of this method reached 100% and it achieved simultaneous editing of three loci with an efficiency of 53.3%. In addition, based on the base editing CRISPR/Cas9n-AID system, we also developed a single plasmid CRISPR/Cas9n system suitable for rapid gene knockout and integration. The knockout efficiency for a single gene reached 93%. Finally, we generated 4 genes (aprE, nprE, wprA, and bamHIR) mutant strain, LB1ba02△4. The mutant strain secreted 1.25-fold more α-amylase into the medium than the wild-type strain.

Conclusions

The CRISPR/Cas9n-AID and CRISPR/Cas9n systems developed in this work proved to be a fast and efficient genetic manipulation tool in a restriction-modification system and poorly transformable strain.

Efficient Genome Editing by a Miniature CRISPR-AsCas12f1 Nuclease in Bacillus anthracis

A miniature CRISPR-Cas12f has been demonstrated to serve as an effective genome editing tool in gram negative bacteria as well as human cells. Here, we developed an alternative method to edit the genome of Bacillus anthracis based on the AsCas12f1 nuclease from Acidibacillus sulfuroxidans. When the htrA gene on the chromosome and the lef gene on the plasmid pXO1 were selected as targets, the CRISPR-AsCas12f1 system showed very high efficiency (100%). At the same time, a high efficiency was observed for large-fragment deletion. Our results also indicated that the length of the homologous arms of the donor DNA had a close relationship with the editing efficiency. Furthermore, a two-plasmid CRISPR-AsCas12f1 system was also constructed and combined with the endonuclease I-SceI for potential multi-gene modification. This represents a novel tool for mutant strain construction and gene function analyses in B. anthracis and other Bacillus cereus group bacteria.

The CRISPR toolbox for the gram-positive model bacterium Bacillus subtilis

CRISPR has revolutionized the way we engineer genomes. Its simplicity and modularity have enabled the development of a great number of tools to edit genomes and to control gene expression. This powerful technology was first adapted to Bacillus subtilis in 2016 and has been intensely upgraded since then. Many tools have been successfully developed to build a CRISPR toolbox for this Gram-positive model and important industrial chassis. The toolbox includes tools, such as double-strand and single-strand cutting CRISPR for point mutation, gene insertion, and gene deletion up to 38 kb. Moreover, catalytic dead Cas proteins have been used for base editing, as well as for the control of gene expression (CRISPRi and CRISPRa). Many of these tools have been used for multiplex CRISPR with the most successful one targeting up to six loci simultaneously for point mutation. However, tools for efficient multiplex CRISPR for other functionalities are still missing in the toolbox. CRISPR engineering has already resulted in efficient protein and metabolite-producing strains, demonstrating its great potential. In this review, we cover all the important additions made to the B. subtilis CRISPR toolbox since 2016, and strain developments fomented by the technology.

The "beauty in the beast"-the multiple uses of Priestia megaterium in biotechnology

Abstract

Over 30 years, the Gram-positive bacterium Priestia megaterium (previously known as Bacillus megaterium) was systematically developed for biotechnological applications ranging from the production of small molecules like vitamin B₁₂, over polymers like polyhydroxybutyrate (PHB) up to the in vivo and in vitro synthesis of multiple proteins and finally whole-cell applications. Here we describe the use of the natural vitamin B₁₂ (cobalamin) producer P. megaterium for the elucidation of the biosynthetic pathway and the subsequent systematic knowledge-based development for production purposes. The formation of PHB, a natural product of P. megaterium and potential petro-plastic substitute, is covered and discussed. Further important biotechnological characteristics of P. megaterium for recombinant protein production including high protein secretion capacity and simple cultivation on value-added carbon sources are outlined. This includes the advanced system with almost 30 commercially available expression vectors for the intracellular and extracellular production of recombinant proteins at the g/L scale. We also revealed a novel P. megaterium transcription-translation system as a complementary and versatile biotechnological tool kit. As an impressive biotechnology application, the formation of various cytochrome P450 is also critically highlighted. Finally, whole cellular applications in plant protection are completing the overall picture of P. megaterium as a versatile giant cell factory.

Key points

• The use of Priestia megaterium for the biosynthesis of small molecules and recombinant proteins through to whole-cell applications is reviewed.

• P. megaterium can act as a promising alternative host in biotechnological production processes.

A SacB-based system for diverse and multiple genome editing in Gluconobacter oxydans

Gluconobacter oxydans is an important industrial bacterial strain widely used to produce a lot of useful products. However, very few gene editing tools are available for G. oxydans. This study aimed to develop an efficient genome editing method for G. oxydans using SacB as a counter-selectable marker. A plasmid that could express the kanamycin resistance gene in both E. coli and G. oxydans was constructed using the screened shuttle promoter P₁₁₆. After optimizing the genome editing conditions, the derivative plasmids could be effectively utilized for diverse genome editing, such as gene deletion, insertion, replacement, and in situ modification in G. oxydans WSH-003. In addition, the SacB-based system also achieved multiple gene editing in G. oxydans. Moreover, the genome of the industrial strain G. oxydans WSH-003 was modified and the growth rate and substrate conversion rate of the strain successfully increased using this system. The system could also have potential to be applied in different G. oxydans strains. The process established in this study also provides a reference for constructing genetic tools for many other genetically recalcitrant bacteria.