Efficient gene editing in Neurospora crassa with CRISPR technology

A user-friendly CRISPR/Cas9 system for mutagenesis of Neurospora crassa

As a widely used eukaryotic model organism, Neurospora crassa offers advantages in genetic studies due to its diverse biology and rapid growth. Traditional genetic manipulation methods, such as homologous recombination, require a considerable amount of time and effort. In this study, we present an easy-to-use CRIPSR/Cas9 system for N. crassa, in which the cas9 sequence is incorporated into the fungal genome and naked guide RNA is introduced via electroporation. Our approach eliminates the need for constructing multiple vectors, speeding up the mutagenesis process. Using cyclosporin-resistant-1 (csr-1) as a selectable marker gene, we achieved 100% editing efficiency under selection conditions. Furthermore, we successfully edited the non-selectable gene N-acylethanolamine amidohydrolase-2 (naa-2), demonstrating the versatility of the system. Combining gRNAs targeting csr-1 and naa-2 simultaneously increased the probability of finding mutants carrying the non-selectable mutation. The system is not only user-friendly but also effective, providing a rapid and efficient method for generating loss-of-function mutants in N. crassa compared to traditional methods.

CRISPR/Cas9 mediated targeted knock-in of eglA gene to improve endoglucanase activity of Aspergillus fumigatus LMB-35Aa

Bioeconomy goals for using biomass feedstock for biofuels and bio-based production has arisen the demand for fungal strains and enzymes for biomass processing. Despite well-known Trichoderma and Aspergillus commercial strains, continuous bioprospecting has revealed the fungal biodiversity potential for production of biomass degrading enzymes. The strain Aspergillus fumigatus LMB-35Aa has revealed a great potential as source of lignocellulose-degrading enzymes. Nevertheless, genetic improvement should be considered to increase its biotechnological potential. Molecular manipulation based on homologous direct recombination (HDR) in filamentous fungi poses a challenge since its low recombination rate. Currently, CRISPR/Cas9-mediated mutagenesis can enable precise and efficient editing of filamentous fungi genomes. In this study, a CRISPR/Cas9-mediated gene editing strategy for improving endoglucanase activity of A. fumigatus LMB-35Aa strain was successfully used, which constitutes the first report of heterologous cellulase production in filamentous fungi using this technology. For this, eglA gene from A. niger ATCC 10,864 was integrated into conidial melanin pksP gene locus, which facilitated the selection of edited events discerned by the emergence of albino colonies. Heterologous production of the EglA enzyme in a biofilm fermentation system resulted in a 40% improvement in endoglucanase activity of the mutant strain compared to the wild type.

Improved Protoplast Production Protocol for Fungal Transformations Mediated by CRISPR/Cas9 in Botrytis cinerea Non-Sporulating Isolates

Botrytis cinerea is a necrotrophic fungus that causes considerable economic losses in commercial crops. Fungi of the genus Botrytis exhibit great morphological and genetic variability, ranging from non-sporogenic and non-infective isolates to highly virulent sporogenic ones. There is growing interest in the different isolates in terms of their methodological applications aimed at gaining a deeper understanding of the biology of these fungal species for more efficient control of the infections they cause. This article describes an improvement in the protoplast production protocol from non-sporogenic isolates, resulting in viable protoplasts with regenerating capacity. The method improvements consist of a two-day incubation period with mycelium plugs and orbital shaking. Special mention is made of our preference for the VinoTaste Pro enzyme in the KC buffer as a replacement for Glucanex, as it enhances the efficacy of protoplast isolation in B459 and B371 isolates. The methodology described here has proven to be very useful for biotechnological applications such as genetic transformations mediated by the CRISPR/Cas9 tool.

Advances in biosynthesis and metabolic engineering strategies of cordycepin

Cordyceps militaris, also called as bei-chong-cao, is an insect-pathogenic fungus from the Ascomycota phylum and the Clavicipitaceae family. It is a valuable filamentous fungus with medicinal and edible properties that has been utilized in traditional Chinese medicine (TCM) and as a nutritious food. Cordycepin is the bioactive compound firstly isolated from C. militaris and has a variety of nutraceutical and health-promoting properties, making it widely employed in nutraceutical and pharmaceutical fields. Due to the low composition and paucity of wild resources, its availability from natural sources is limited. With the elucidation of the cordycepin biosynthetic pathway and the advent of synthetic biology, a green cordycepin biosynthesis in Saccharomyces cerevisiae and Metarhizium robertsii has been developed, indicating a potential sustainable production method of cordycepin. Given that, this review primarily focused on the metabolic engineering and heterologous biosynthesis strategies of cordycepin.

Efficient gene editing in the slow-growing, non-sporulating, melanized, endophytic fungus Berkleasmium sp. Dzf12 using a CRISPR/Cas9 system

The endophytic fungus Berkleasmium sp. Dzf12 that was isolated from Dioscorea zingiberensis, is a proficient producer of palmarumycins, which are intriguing polyketides of the spirobisnaphthalene class. These compounds displayed a wide range of bioactivities, including antibacterial, antifungal, and cytotoxic activities. However, conventional genetic manipulation of Berkleasmium sp. Dzf12 is difficult and inefficient, partially due to the slow-growing, non-sporulating, and highly pigmented behavior of this fungus. Herein, we developed a CRISPR/Cas9 system suitable for gene editing in Berkleasmium sp. Dzf12. The protoplast preparation was optimized, and the expression of Cas9 in Berkleasmium sp. Dzf12 was validated. To assess the gene disruption efficiency, a putative 1, 3, 6, 8-tetrahydroxynaphthalene synthase encoding gene, bdpks, involved in 1,8-dihydroxynaphthalene (DHN)-melanin biosynthesis, was selected as the target for gene disruption. Various endogenous sgRNA promoters were tested, and different strategies to express sgRNA were compared, resulting in the construction of an optimal system using the U6 snRNA-1 promoter as the sgRNA promoter. Successful disruption of bdpks led to a complete abolishment of the production of spirobisnaphthalenes and melanin. This work establishes a useful gene targeting disruption system for exploration of gene functions in Berkleasmium sp. Dzf12, and also provides an example for developing an efficient CRISPR/Cas9 system to the fungi that are difficult to manipulate using conventional genetic tools.

Utilization of CRISPR-Cas genome editing technology in filamentous fungi: function and advancement potentiality

Filamentous fungi play a crucial role in environmental pollution control, protein secretion, and the production of active secondary metabolites. The evolution of gene editing technology has significantly improved the study of filamentous fungi, which in the past was laborious and time-consuming. But recently, CRISPR-Cas systems, which utilize small guide RNA (sgRNA) to mediate clustered regularly interspaced short palindromic repeats (CRISPR) and CRISPR-associated proteins (Cas), have demonstrated considerable promise in research and application for filamentous fungi. The principle, function, and classification of CRISPR-Cas, along with its application strategies and research progress in filamentous fungi, will all be covered in the review. Additionally, we will go over general matters to take into account when editing a genome with the CRISPR-Cas system, including the creation of vectors, different transformation methodologies, multiple editing approaches, CRISPR-mediated transcriptional activation (CRISPRa) or interference (CRISPRi), base editors (BEs), and Prime editors (PEs).

Recyclable CRISPR/Cas9-mediated gene disruption and deletions in Histoplasma

IMPORTANCE

Histoplasma is a primary fungal pathogen with the ability to infect otherwise healthy mammalian hosts, causing systemic and sometimes life-threatening disease. Thus far, molecular genetic manipulation of this organism has utilized RNA interference, random insertional mutagenesis, and a homologous recombination protocol that is highly variable and often inefficient. Targeted gene manipulations have been challenging due to poor rates of homologous recombination events in Histoplasma. Interrogation of the virulence strategies of this organism would be highly accelerated by a means of efficiently generating targeted mutations. We have developed a recyclable CRISPR/Cas9 system that can be used to introduce gene disruptions in Histoplasma with high efficiency, thereby allowing disruption of multiple genes.

A journey with psychedelic mushrooms: From historical relevance to biology, cultivation, medicinal uses, biotechnology, and beyond

Psychedelic mushrooms containing psilocybin and related tryptamines have long been used for ethnomycological purposes, but emerging evidence points to the potential therapeutic value of these mushrooms to address modern neurological, psychiatric health, and related disorders. As a result, psilocybin containing mushrooms represent a re-emerging frontier for mycological, biochemical, neuroscience, and pharmacology research. This work presents crucial information related to traditional use of psychedelic mushrooms, as well as research trends and knowledge gaps related to their diversity and distribution, technologies for quantification of tryptamines and other tryptophan-derived metabolites, as well as biosynthetic mechanisms for their production within mushrooms. In addition, we explore the current state of knowledge for how psilocybin and related tryptamines are metabolized in humans and their pharmacological effects, including beneficial and hazardous human health implications. Finally, we describe opportunities and challenges for investigating the production of psychedelic mushrooms and metabolic engineering approaches to alter secondary metabolite profiles using biotechnology integrated with machine learning. Ultimately, this critical review of all aspects related to psychedelic mushrooms represents a roadmap for future research efforts that will pave the way to new applications and refined protocols.

Development of CRISPR/Cas9-Based Genome Editing Tools for Polyploid Yeast Cyberlindnera jadinii and Its Application in Engineering Heterologous Steroid-Producing Strains

In this study, a suite of efficient CRISPR/Cas9 tools was developed to overcome the genetic manipulation challenges posed by the polyploid genome of industrial yeast Cyberlindnera jadinii. The developed CRISPR/Cas9 system can achieve a 100% single-gene knockdown efficiency in strain NBRC0988. Moreover, the integration of a single exogenous gene into the target locus using a 50 bp homology arm achieved near-100% efficiency. The efficiency of simultaneous integration of three genes into the chromosome is strongly influenced by the length of the homology arm, with the highest integration efficiency of 62.5% obtained when selecting a homology arm of about 500 bp. By utilizing the CRISPR/Cas system, this study demonstrated the potential of C. jadinii in producing heterologous sterols. Through shake-flask fermentation, the engineered strains produced 92.1 and 81.8 mg/L of campesterol and cholesterol, respectively. Furthermore, the production levels of these two sterols were further enhanced through high-cell-density fed-batch fermentation in a 5 L bioreactor. The highest titer of campesterol reached 807 mg/L [biomass OD600 = 294, productivity of 6.73 mg/(L·h)]. The titer of cholesterol reached 1.52 g/L [biomass OD600 = 380, productivity of 9.06 mg/(L·h)], marking the first gram-scale production of steroidal compounds in C. jadinii.

Simplified and effective RNA interference and CRISPR-Cas9 systems for Cryptococcus neoformans

The 3,4-dihydroxyphenylalanine (DOPA) melanin is one of the important virulence factors for Cryptococcus neoformans, which may trigger immune responses in the host. While the production of DOPA melanin is catalyzed by laccase that is predominantly encoded by LAC1 gene. Therefore, regulating the genetic expression of C. neoformans is conducive to exploring the impact of interested molecules on the host. In this work, we established two systems that were constructed quickly and easily for the knock-down/knock-out of LAC1 gene: RNA interference (RNAi) and clustered regularly interspaced short palindromic repeats CRISPR-Cas9. The RNAi system was constructed by pSilencer 4.1-CMV neo plasmid and short hairpin RNA to achieve effective transcriptional suppression. The CRISPR-Cas9 system was used the PNK003 vectors to obtain a stable albino mutant strain. The results of phenotype, quantitative real-time polymerase chain reaction, transmission electron microscope, and spectrophotometry were used to assess the ability of melanin production. As a result, the RNAi system displayed attenuation of transcriptional suppression when the transformants continuously passed on new plates. However, the transcriptional suppression of long loop in short hairpin RNA was more powerful and lasted longer. An albino strain produced by CRISPR-Cas9 was completely unable to synthesize melanin. In conclusion, strains with different capacities of melanin production were obtained by RNAi and CRISPR-Cas9 systems, which might be useful for exploring the linear relation between melanin and immunoreaction of the host. In addition, the two systems in this article might be convenient to quickly screen the possible trait-regulating genes of other serotypes of C. neoformans.

CRISPR/Cas9 mediated gene editing of transcription factor ACE1 for enhanced cellulase production in thermophilic fungus Rasamsonia emersonii

BACKGROUND

The filamentous fungus Rasamsonia emersonii has immense potential to produce biorefinery relevant thermostable cellulase and hemicellulase enzymes using lignocellulosic biomass. Previously in our lab, a hyper-cellulase producing strain of R. emersonii was developed through classical breeding and system biology approaches. ACE1, a pivotal transcription factor in fungi, plays a crucial role in negatively regulating the expression of cellulase genes. In order to identify the role of ACE1 in cellulase production and to further improve the lignocellulolytic enzyme production in R. emersonii, CRISPR/Cas9 mediated disruption of ACE1 gene was employed.

RESULTS

A gene-edited ∆ACE1 strain (GN11) was created, that showed 21.97, 20.70 and 24.63, 9.42, 18.12%, improved endoglucanase, cellobiohydrolase (CBHI), β-glucosidase, FPase, and xylanase, activities, respectively, as compared to parental strain M36. The transcriptional profiling showed that the expression of global regulator (XlnR) and different CAZymes genes including endoglucanases, cellobiohydrolase, β-xylosidase, xylanase, β-glucosidase and lytic polysaccharide mono-oxygenases (LPMOs) were significantly enhanced, suggesting critical roles of ACE1 in negatively regulating the expression of various key genes associated with cellulase production in R. emersonii. Whereas, the disruption of ACE1 significantly down-regulated the expression of CreA repressor gene as also evidenced by 2-deoxyglucose (2-DG) resistance phenotype exhibited by edited strain GN11 as well as appreciably higher constitutive production of cellulases in the presence of glucose and mixture of glucose and disaccharide (MGDs) both in batch and flask fed batch mode of culturing. Furthermore, ∆ACE1 strains were evaluated for the hydrolysis of biorefinery relevant steam/acid pretreated unwashed rice straw slurry (Praj Industries Ltd; 15% substrate loading rate) and were found to be significantly superior when compared to the benchmark enzymes produced by parent strain M36 and Cellic Ctec3.

CONCLUSIONS

Current work uncovers the crucial role of ACE1 in regulating the expression of the various cellulase genes and carbon catabolite repression mechanism in R. emersonii. This study represents the first successful report of utilizing CRISPR/Cas9 genome editing technology to disrupt the ACE1 gene in the thermophlic fungus R. emersonii. The improved methodologies presented in this work might be applied to other commercially important fungal strains for which genetic manipulation tools are limited.

Identification of a common secondary mutation in the Neurospora crassa knockout collection conferring a cell fusion-defective phenotype

Gene-deletion mutants represent a powerful tool to study gene function. The filamentous fungus Neurospora crassa is a well-established model organism, and features a comprehensive gene knockout strain collection. While these mutant strains have been used in numerous studies, resulting in the functional annotation of many Neurospora genes, direct confirmation of gene-phenotype relationships is often lacking, which is particularly relevant given the possibility of background mutations, sample contamination, and/or strain mislabeling. Indeed, spontaneous mutations resulting in phenotypes resembling many cell fusion mutants have long been known to occur at relatively high frequency in N. crassa, and these secondary mutations are common in the Neurospora deletion collection. The identity of these mutations, however, is largely unknown. Here, we report that the Δada-3 strain from the N. crassa knockout collection, which exhibits a cell fusion defect, harbors a secondary mutation responsible for this phenotype. Through whole-genome sequencing and genetic analyses, we found a ~30-Kb deletion in this strain affecting a known cell fusion-related gene, so/ham-1, and show that it is the absence of this gene-and not of ada-3-that underlies its cell fusion defect. We additionally found three other knockout strains harboring the same deletion, suggesting that this mutation may be common in the collection and could have impacted previous studies. Our findings provide a cautionary note and highlight the importance of proper functional validation of strains from mutant collections. We discuss our results in the context of the spread of cell fusion-defective cheater variants in N. crassa cultures. IMPORTANCE This study emphasizes the need for careful and detailed characterization of strains from mutant collections. Specifically, we found a common deletion in various strains from the Neurospora crassa gene knockout collection that results in a cell fusion-defective phenotype. This is noteworthy because this collection is known to contain background mutations-of a largely unclear nature-that produce cell fusion-defective phenotypes. Our results describe an example of such mutations, and highlight how this common genetic defect could have impacted previous studies that have used the affected strains. Furthermore, they provide a cautionary note about the use of Neurospora strains with similar phenotypes. Lastly, these findings offer additional details relevant to our understanding of the origin and spread of cell fusion-defective cheater variants in N. crassa cultures.

Strategies for the Development of Industrial Fungal Producing Strains

The use of microorganisms in industry has enabled the (over)production of various compounds (e.g., primary and secondary metabolites, proteins and enzymes) that are relevant for the production of antibiotics, food, beverages, cosmetics, chemicals and biofuels, among others. Industrial strains are commonly obtained by conventional (non-GMO) strain improvement strategies and random screening and selection. However, recombinant DNA technology has made it possible to improve microbial strains by adding, deleting or modifying specific genes. Techniques such as genetic engineering and genome editing are contributing to the development of industrial production strains. Nevertheless, there is still significant room for further strain improvement. In this review, we will focus on classical and recent methods, tools and technologies used for the development of fungal production strains with the potential to be applied at an industrial scale. Additionally, the use of functional genomics, transcriptomics, proteomics and metabolomics together with the implementation of genetic manipulation techniques and expression tools will be discussed.

Epigenetic manipulation for secondary metabolite activation in endophytic fungi: current progress and future directions

Fungal endophytes have emerged as a promising source of secondary metabolites with significant potential for various applications in the field of biomedicine. The biosynthetic gene clusters of endophytic fungi are responsible for encoding several enzymes and transcriptional factors that are involved in the biosynthesis of secondary metabolites. The investigation of fungal metabolic potential at genetic level faces certain challenges, including the synthesis of appropriate amounts of chemicals, and loss of the ability of fungal endophytes to produce secondary metabolites in an artificial culture medium. Therefore, there is a need to delve deeper into the field of fungal genomics and transcriptomics to explore the potential of fungal endophytes in generating secondary metabolites governed by biosynthetic gene clusters. The silent biosynthetic gene clusters can be activated by modulating the chromatin structure using chemical compounds. Epigenetic modification plays a significant role by inducing cryptic gene responsible for the production of secondary metabolites using DNA methyl transferase and histone deacetylase. CRISPR-Cas9-based genome editing emerges an effective tool to enhance the production of desired metabolites by modulating gene expression. This review primarily focuses on the significance of epigenetic elicitors and their capacity to boost the production of secondary metabolites from endophytes. This article holds the potential to rejuvenate the drug discovery pipeline by introducing new chemical compounds.

Establishment of a genome editing tool using CRISPR-Cas9 ribonucleoprotein complexes in the non-model plant pathogen Sphaerulina musiva

CRISPR-Cas9 is a versatile genome editing system widely used since 2013 to introduce site-specific modifications into the genomes of model and non-model species. This technology is used in various applications, from gene knock-outs, knock-ins, and over-expressions to more precise changes, such as the introduction of nucleotides at a targeted locus. CRISPR-Cas9 has been demonstrated to be easy to establish in new species and highly efficient and specific compared to previous gene editing strategies such as Zinc finger nucleases and transcription activator-like effector nucleases. Grand challenges for emerging CRISPR-Cas9 tools in filamentous fungi are developing efficient transformation methods for non-model organisms. In this paper, we have leveraged the establishment of CRISPR-Cas9 genome editing tool that relies on Cas9/sgRNA ribonucleoprotein complexes (RNPs) in the model species Trichoderma reesei and developed the first protocol to efficiently transform the non-model species, Sphaerulina musiva. This fungal pathogen constitutes a real threat to the genus Populus, a foundational bioenergy crop used for biofuel production. Herein, we highlight the general considerations to design sgRNAs and their computational validation. We also describe the use of isolated protoplasts to deliver the CRISPR-Cas9 RNP components in both species and the screening for targeted genome editing events. The development of engineering tools in S. musiva can be used for studying genes involved in diverse processes such as secondary metabolism, establishment, and pathogenicity, among many others, but also for developing genetic mitigation approaches. The approach described here provides guidance for potential development of transformation systems in other non-model spore-bearing ascomycetes.

Recyclable CRISPR/Cas9 mediated gene disruption and deletions in Histoplasma

Targeted gene disruption is challenging in the dimorphic fungal pathogen Histoplasma due to the low frequency of homologous recombination. Transformed DNA is either integrated ectopically into the genome or maintained extra chromosomally by de novo addition of telomeric sequences. Based on a system developed in Blastomyces, we adapted a CRISPR/Cas9 system to facilitate targeted gene disruption in Histoplasma with high efficiency. We express a codon-optimized version of Cas9 as well as guide RNAs from a single ectopic vector carrying a selectable marker. Once the desired mutation is verified, one can screen for isolates that have lost the Cas9 vector by simply removing the selective pressure. Multiple mutations can then be generated in the same strain by retransforming the Cas9 vector carrying different guides. We used this system to disrupt a number of target genes including RYP2 and SRE1 where loss-of-function mutations could be monitored visually by colony morphology or color, respectively. Interestingly, expression of two guide RNAs targeting the 5' and 3' ends of a gene allowed isolation of deletion mutants where the sequence between the guide RNAs was removed from the genome. Whole-genome sequencing showed that the frequency of off-target mutations associated with the Cas9 nuclease was negligible. Finally, we increased the frequency of gene disruption by using an endogenous Histoplasma regulatory sequence to drive guide RNA expression. These tools transform our ability to generate targeted mutations in Histoplasma.

Generation of CRISPR-Cas9-mediated knockin mutant models in mice and MEFs for studies of polymorphism in clock genes

The creation of mutant mice has been invaluable for advancing biomedical science, but is too time- and resource-intensive for investigating the full range of mutations and polymorphisms. Cell culture models are therefore an invaluable complement to mouse models, especially for cell-autonomous pathways like the circadian clock. In this study, we quantitatively assessed the use of CRISPR to create cell models in mouse embryonic fibroblasts (MEFs) as compared to mouse models. We generated two point mutations in the clock genes Per1 and Per2 in mice and in MEFs using the same sgRNAs and repair templates for HDR and quantified the frequency of the mutations by digital PCR. The frequency was about an order of magnitude higher in mouse zygotes compared to that in MEFs. However, the mutation frequency in MEFs was still high enough for clonal isolation by simple screening of a few dozen individual cells. The Per mutant cells that we generated provide important new insights into the role of the PAS domain in regulating PER phosphorylation, a key aspect of the circadian clock mechanism. Quantification of the mutation frequency in bulk MEF populations provides a valuable basis for optimizing CRISPR protocols and time/resource planning for generating cell models for further studies.

State of the Art of the Molecular Biology of the Interaction between Cocoa and Witches’ Broom Disease: A Systematic Review

Significant scientific advances to elucidate the Moniliophthora perniciosa pathosystem have been achieved in recent years, but the molecular biology of this pathogen-host interaction is still a field with many unanswered questions. In order to present insights at the molecular level, we present the first systematic review on the theme. All told, 1118 studies were extracted from public databases. Of these, 109 were eligible for the review, based on the inclusion and exclusion criteria. The results indicated that understanding the transition from the biotrophic-necrotrophic phase of the fungus is crucial for control of the disease. Proteins with strong biotechnological potential or that can be targets for pathosystem intervention were identified, but studies regarding possible applications are still limited. The studies identified revealed important genes in the M. perniciosa-host interaction and efficient molecular markers in the search for genetic variability and sources of resistance, with Theobroma cacao being the most common host. An arsenal of effectors already identified and not explored in the pathosystem were highlighted. This systematic review contributes to the understanding of the pathosystem at the molecular level, offering new insights and proposing different paths for the development of new strategies to control witches’ broom disease.

Bioengineering of fungal endophytes through the CRISPR/Cas9 system

The CRISPR/Cas9 system is a genome-editing tool that allows for precise and efficient modifications to the DNA of a cell. This technology can be used in endophytic fungi, which live within plants and can have beneficial effects on their host, making them important for agriculture. Using CRISPR/Cas9, researchers can introduce specific genetic changes into endophytic fungal genomes, allowing them to study the function of genes, improve their plant-growth-promoting properties, and create new, more beneficial endophytes. This system works by using the Cas9 protein, which acts as a pair of molecular scissors, to cut DNA at specific locations determined by a guide RNA. Once the DNA is cut, the cell’s natural repair mechanisms can be used to insert or delete specific genes, allowing for precise editing of the fungal genome. This article discusses the mechanism and applications of CRISPR/Cas9 to fungal endophytes.

Developing a Temperature-Inducible Transcriptional Rheostat in Neurospora crassa

Heat shock protein (HSP)-encoding genes (hsp), part of the highly conserved heat shock response (HSR), are known to be induced by thermal stress in several organisms. In Neurospora crassa, three hsp genes, hsp30, hsp70, and hsp80, have been characterized; however, the role of defined cis elements in their responses to discrete changes in temperature remains largely unexplored. To fill this gap, while also aiming to obtain a reliable fungal heat shock-inducible system, we analyzed different sections of each hsp promoter by assessing the expression of real-time transcriptional reporters. Whereas all three promoters and their resected versions were acutely induced by high temperatures, only hsp30 displayed a broad range of expression and high tunability, amply exceeding other inducible promoter systems existing in Neurospora, such as quinic acid- or light-inducible ones. As proof of concept, we employed one of these promoters to control the expression of clr-2, which encodes the master regulator of Neurospora cellulolytic capabilities. The resulting strain fails to grow on cellulose at 25°C, whereas it grows robustly if heat shock pulses are delivered daily. Additionally, we designed two hsp30 synthetic promoters and characterized them, as well as the native promoters, using a gradient of high temperatures, yielding a wide range of responses to thermal stimuli. Thus, Neurospora hsp30-based promoters represent a new set of modular elements that can be used as transcriptional rheostats to adjust the expression of a gene of interest or for the implementation of regulated circuitries for synthetic biology and biotechnological strategies. IMPORTANCE A timely and dynamic response to strong temperature fluctuations is paramount for organismal biology. At the same time, inducible promoters are a powerful tool for fungal biotechnological and synthetic biology endeavors. In this work, we analyzed the activity of several N. crassa heat shock protein (hsp) promoters at a wide range of temperatures, observing that hsp30 exhibits remarkable sensitivity and a dynamic range of expression as we charted the response of this promoter to subtle increases in temperature, and also as we built and analyzed synthetic promoters based on hsp30 cis elements. As proof of concept, we tested the ability of hsp30 to provide tight control of a central process, cellulose degradation. While this study provides an unprecedented description of the regulation of the N. crassa hsp genes, it also contributes a noteworthy addition to the molecular toolset of transcriptional controllers in filamentous fungi.

Endogenous circadian reporters reveal functional differences of PERIOD paralogs and the significance of PERIOD:CK1 stable interaction

Adverse consequences from having a faulty circadian clock include compromised sleep quality and poor performance in the short-term, and metabolic diseases and cancer in the long-term. However, our understanding of circadian disorders is limited by the incompleteness of our molecular models and our dearth of defined mutant models. Because it would be prohibitively expensive to develop live animal models to study the full range of complicated clock mechanisms, we developed PER1-luc and PER2-luc endogenous circadian reporters in a validated clock cell model, U-2 OS, where the genome can be easily manipulated, and functional consequences of mutations can be accurately studied. When major clock genes were knocked out in these cells, circadian rhythms were modulated similarly compared with corresponding mutant mice, validating the platform for genetics studies. Using these reporter cells, we uncovered critical differences between two paralogs of PER. Although PER1 and PER2 are considered redundant and either one can serve as a pacemaker alone, they were dramatically different in biochemical parameters such as stability and phosphorylation kinetics. Consistently, circadian phase was dramatically different between PER1 and PER2 knockout reporter cells. We further showed that the stable binding of casein kinase1δ/ε to PER is not required for PER phosphorylation itself, but is critical for delayed timing of phosphorylation. Our system can be used as an efficient platform to study circadian disorders associated with pathogenic mutations and their underlying molecular mechanisms.

Current advancement in the application of prime editing

Prime editing (PE) is a precise genome manipulation technology based on the "search and replace" approach of the CRISPR-Cas9 system, while it does not require the exogenous donor DNA and the DNA double-strand breaks (DSBs). Comparing the base editing technology, the editing scope of prime editing has been widely expanded. Prime editing has been successfully applied in a variety of plant cells, animal cells and the model microorganism Escherichia coli so far, and it has shown a good application potential in breeding and genomic functional study of animals and plants, disease treatment, and modification of the microbial strains. In this paper, the basic strategies of prime editing are briefly described, and its research progress is summarized and prospected from the application of multiple species. In addition, a variety of optimization strategies for improving its efficiency and specificity of prime editing are outlined.

Industrial applications of fungal lipases: a review

Fungal lipases (triacylglycerol acyl hydrolases EC 3.1.1.3) are significant industrial enzymes and have several applications in a number of industries and fields. Fungal lipases are found in several species of fungi and yeast. These enzymes are carboxylic acid esterases, categorized under the serine hydrolase family, and do not require any cofactor during the catalyzing of the reactions. It was also noticed that processes including the extraction and purification of lipases from fungi are comparatively easier and cheaper than other sources of lipases. In addition, fungal lipases have been classified into three chief classes, namely, GX, GGGX, and Y. Fungal lipases have applications not only in the hydrolysis of fats and oils (triglycerides) but are also involved in synthetic reactions such as esterification, acidolysis, alcoholysis, interesterification, and aminolysis. The production and activity of fungal lipases are highly affected by the carbon source, nitrogen source, temperature, pH, metal ions, surfactants, and moisture content. Therefore, fungal lipases have several industrial and biotechnological applications in many fields such as biodiesel production, ester synthesis, production of biodegradable biopolymers, formulations of cosmetics and personal care products, detergent manufacturing, degreasing of leather, pulp and paper production, textile industry, biosensor development, and drug formulations and as a diagnostic tool in the medical sector, biodegradation of esters, and bioremediation of wastewater. The immobilization of fungal lipases onto different carriers also helps in improving the catalytic activities and efficiencies of lipases by increasing thermal and ionic stability (in organic solvents, high pH, and temperature), being easy to recycle, and inducing the volume-specific loading of the enzyme onto the support, and thus, these features have proved to be appropriate for use as biocatalysts in different sectors.

Editing Aspergillus terreus using the CRISPR-Cas9 system

CRISPR-Cas9 technology has been utilized in different organisms for targeted mutagenesis, offering a fast, precise and cheap approach to speed up molecular breeding and study of gene function. Until now, many researchers have established the demonstration of applying the CRISPR/Cas9 system to various fungal model species. However, there are very few guidelines available for CRISPR/Cas9 genome editing in Aspergillus terreus. In this study, we present CRISPR/Cas9 genome editing in A. terreus. To optimize the guide ribonucleic acid (gRNA) expression, we constructed a modified single-guide ribonucleic acid (sgRNA)/Cas9 expression plasmid. By co-transforming an sgRNA/Cas9 expression plasmid along with maker-free donor deoxyribonucleic acid (DNA), we precisely disrupted the lovB and lovR genes, respectively, and created targeted gene insertion (lovF gene) and iterative gene editing in A. terreus (lovF and lovR genes). Furthermore, co-delivering two sgRNA/Cas9 expression plasmids resulted in precise gene deletion (with donor DNA) in the ku70 and pyrG genes, respectively, and efficient removal of the DNA between the two gRNA targeting sites (no donor DNA) in the pyrG gene. Our results showed that the CRISPR/Cas9 system is a powerful tool for precise genome editing in A. terreus, and our approach provides a great potential for manipulating targeted genes and contributions to gene functional study of A. terreus.

A detailed landscape of CRISPR-Cas-mediated plant disease and pest management

Genome editing technology has rapidly evolved to knock-out genes, create targeted genetic variation, install precise insertion/deletion and single nucleotide changes, and perform large-scale alteration. The flexible and multipurpose editing technologies have started playing a substantial role in the field of plant disease management. CRISPR-Cas has reduced many limitations of earlier technologies and emerged as a versatile toolbox for genome manipulation. This review summarizes the phenomenal progress of the use of the CRISPR toolkit in the field of plant pathology. CRISPR-Cas toolbox aids in the basic studies on host-pathogen interaction, in identifying virulence genes in pathogens, deciphering resistance and susceptibility factors in host plants, and engineering host genome for developing resistance. We extensively reviewed the successful genome editing applications for host plant resistance against a wide range of biotic factors, including viruses, fungi, oomycetes, bacteria, nematodes, insect pests, and parasitic plants. Recent use of CRISPR-Cas gene drive to suppress the population of pathogens and pests has also been discussed. Furthermore, we highlight exciting new uses of the CRISPR-Cas system as diagnostic tools, which rapidly detect pathogenic microorganism. This comprehensive yet concise review discusses innumerable strategies to reduce the burden of crop protection.

Development of Genetic Tools in Glucoamylase-Hyperproducing Industrial Aspergillus niger Strains

Simple Summary

Glucoamylase is one of the most needed industrial enzymes in the food and biofuel industries. Aspergillus niger is a commonly used cell factory for the production of commercial glucoamylase. For decades, genetic manipulation has promoted significant progress in industrial fungi for strain engineering and in obtaining deep insights into their genetic features. However, genetic engineering is more laborious in the glucoamylase-producing industrial strains A. niger N1 and O1 because their fungal features of having few conidia (N1) or of being aconidial (O1) make them difficult to perform transformation on. In this study, we targeted A. niger N1 and O1 and successfully developed high-efficiency transformation tools. We also constructed a clustered regularly interspaced short palindromic repeat (CRISPR)/Cas9 editing marker-free system using an autonomously replicating plasmid to express Cas9 protein and to guide RNA and the selectable marker. By using the genetic tools developed here, we generated nine albino deletion mutants. After three rounds of sub-culturing under nonselective conditions, the albino deletions lost the autonomously replicating plasmid. Together, the tools and optimization process above provided a good reference to manipulate the tough working industrial strain, not only for the further engineering these two glucoamylase-hyperproducing strains, but also for other industrial strains.

Abstract

The filamentous fungus Aspergillus niger is widely exploited by the fermentation industry for the production of enzymes, particularly glucoamylase. Although a variety of genetic techniques have been successfully used in wild-type A. niger, the transformation of industrially used strains with few conidia (e.g., A. niger N1) or that are even aconidial (e.g., A. niger O1) remains laborious. Herein, we developed genetic tools, including the protoplast-mediated transformation and Agrobacterium tumefaciens-mediated transformation of the A. niger strains N1 and O1 using green fluorescent protein as a reporter marker. Following the optimization of various factors for protoplast release from mycelium, the protoplast-mediated transformation efficiency reached 89.3% (25/28) for N1 and 82.1% (32/39) for O1. The A. tumefaciens-mediated transformation efficiency was 98.2% (55/56) for N1 and 43.8% (28/64) for O1. We also developed a marker-free CRISPR/Cas9 genome editing system using an AMA1-based plasmid to express the Cas9 protein and sgRNA. Out of 22 transformants, 9 albA deletion mutants were constructed in the A. niger N1 background using the protoplast-mediated transformation method and the marker-free CRISPR/Cas9 system developed here. The genome editing methods improved here will accelerate the elucidation of the mechanism of glucoamylase hyperproduction in these industrial fungi and will contribute to the use of efficient targeted mutation in other industrial strains of A. niger.

Breeding Tools for Assessing and Improving Resistance and Limiting Mycotoxin Production by Fusarium graminearum in Wheat

The recently adopted conservation and minimum tillage practices in wheat-production systems coupled with the concomitant warming of the Earth are believed to have caused the upsurges in Fusarium head blight (FHB) prevalence in major wheat-producing regions of the world. Measures to counter this effect include breeding for resistance to both initial infection of wheat and spread of the disease. Cases of mycotoxicosis caused by ingestion of wheat by-products contaminated with FHB mycotoxins have necessitated the need for resistant wheat cultivars that can limit mycotoxin production by the dominant causal pathogen, Fusarium graminearum. This manuscript reviews breeding tools for assessing and improving resistance as well as limiting mycotoxin contamination in wheat to reflect on the current state of affairs. Combining these aspects in wheat research and development promotes sustainable quality grain production and safeguards human and livestock health from mycotoxicosis.

Employment of the CRISPR/Cas9 system to improve cellulase production in Trichoderma reesei

Trichoderma reesei has been explored intensively in the laboratory and on an industrial scale for its highly potent cellulase secretion machinery since its characterization over 70 years ago. Emergence of new genetic tools over the past decade has strengthened the understanding of mechanism involved in transcription of cellulase genes in fungi and provided a boost to edit them at molecular level. Since several transcriptional factors work synergistically for cellulase expression in fungi; engineering of cellulase secretome for enhanced cellulase titer require combined manipulation of these factors. In the same context, CRISPR/Cas9 has emerged as a powerful, versatile genetic engineering tool for multiplex gene editing in fungi. It is true that considerable efforts with CRISPR technologies have largely developed fungal genetic engineering, but its application in fungi is still challenging and limited. The present review illustrates the precision, strengths and challenges of using CRISPR/Cas9 technology for cellulase engineering in T. reesei, highlighting key strategies that could be employed for strain improvement.

Development of the CRISPR-Cas9 System for the Marine-Derived Fungi Spiromastix sp. SCSIO F190 and Aspergillus sp. SCSIO SX7S7

Marine-derived fungi are emerging as attractive producers of structurally novel secondary metabolites with diverse bioactivities. However, the lack of efficient genetic tools limits the discovery of novel compounds and the elucidation of biosynthesis mechanisms. Here, we firstly established an effective PEG-mediated chemical transformation system for protoplasts in two marine-derived fungi, Spiromastix sp. SCSIO F190 and Aspergillus sp. SCSIO SX7S7. Next, we developed a simple and versatile CRISPR-Cas9-based gene disruption strategy by transforming a target fungus with a single plasmid. We found that the transformation with a circular plasmid encoding cas9, a single-guide RNA (sgRNA), and a selectable marker resulted in a high frequency of targeted and insertional gene mutations in both marine-derived fungal strains. In addition, the histone deacetylase gene rpd3 was mutated using the established CRISPR-Cas9 system, thereby activating novel secondary metabolites that were not produced in the wild-type strain. Taken together, a versatile CRISPR-Cas9-based gene disruption method was established, which will promote the discovery of novel natural products and further biological studies.

Efficient multiplex CRISPR/Cpf1 (Cas12a) genome editing system in Aspergillus aculeatus TBRC 277

CRISPR/Cas technology is a versatile tool for genome engineering in many organisms, including filamentous fungi. Cpf1 is a multi-domain protein of class 2 (type V) RNA-guided CRISPR/Cas endonuclease, and is an alternative platform with distinct features when compared to Cas9. However, application of this technology in filamentous fungi is limited. Here, we present a single CRISPR/Cpf1 plasmid system in Aspergillus aculeatus strain TBRC 277, an industrially relevant cell factory. We first evaluated the functionality of three Cpf1 orthologs from Acidaminococcus sp. BV3L6 (AsCpf1), Francisella tularensis subsp. novicida U112 (FnCpf1), and Lachnospiraceae bacterium (LbCpf1), in RNA-guided site-specific DNA cleavage at the pksP locus. FnCpf1 showed the highest editing efficiency (93%) among the three Cpf1s. It was further investigated for its ability to delete a 1.7kb and a 0.5kb from pksP and pyrG genes, respectively, using two protospacers targeting these gene loci in a single crRNA array. Lastly, simultaneous editing of three sites within TBRC 277 genome was performed using three guide sequences targeting these two genes as well as an additional gene, kusA, which resulted in combined editing efficiency of 40%. The editing of the NHEJ pathway by targeting kusA to generate a NHEJ-deficient strain of A. aculeatus TBRC 277 improved gene targeting efficiency and yielded more precise gene-editing than that of using wild-type strain. This promising genome-editing system can be used for strain improvement in industrial applications such as production of valuable bioproducts.

Genome editing using preassembled CRISPR-Cas9 ribonucleoprotein complexes in Fusarium graminearum

Genome editing using the clustered regularly interspaced short palindromic repeats (CRISPR)-CRISPR-associated protein 9 (Cas9) system has greatly facilitated the genetic analysis of fungal pathogens. The head blight fungus, Fusarium graminearum, causes destructive losses of economically important cereal crops. The recent development of the CRISPR-Cas9 system for use with F. graminearum has enabled more efficient genome editing. In this study, we described a CRISPR-Cas9-based genome-editing tool for the direct delivery of preassembled Cas9 ribonucleoproteins (RNPs) into the protoplasts of F. graminearum. The use of RNPs significantly increased both the number of transformants and percentage of transformants in which the target gene was successfully replaced with a selectable marker. We showed that a single double-strand DNA break mediated by the Cas9 ribonucleoprotein was sufficient for gene deletion. In addition, short-homology recombination required only 50 base pair regions flanking the target gene. The high efficiency of Cas9 RNPs enables large-scale functional analysis, the identification of essential genes, and gene deletion that is difficult with conventional methods. We expect that our approach will accelerate genetic studies of F. graminearum.

Development of an Efficient C-to-T Base-Editing System and Its Application to Cellulase Transcription Factor Precise Engineering in Thermophilic Fungus Myceliophthora thermophila

Myceliophthora thermophila is a thermophilic fungus with great potential in biorefineries and biotechnology. The base editor is an upgraded version of the clustered regularly interspaced short palindromic repeats (CRISPR)-dependent genome-editing tool that introduces precise point mutations without causing DNA double-strand breaks (DSBs) and has been used in various organisms but rarely in filamentous fungi, especially thermophilic filamentous fungi. Here, for the first time, we constructed three cytosine base editors (CBEs) in M. thermophila, namely, evolved apolipoprotein B mRNA-editing enzyme catalytic subunit 1 (APOBEC1) cytosine base editor 4 max (Mtevo-BE4max), bacteriophage Mu Gam protein cytosine base editor 4 max (MtGAM-BE4max), and evolved CDA1 deaminase cytosine base editor (Mtevo-CDA1), and efficiently inactivated genes by precisely converting three codons (CAA, CAG, and CGA) into stop codons without DSB formation. The Mtevo-CDA1 editor with up to 92.6% editing efficiency is a more suitable tool for cytosine base editing in thermophilic fungi. To investigate the function of each motif of the cellulase transcription factor M. thermophila CLR-2 (MtCLR-2), we used the Mtevo-CDA1 editor. The fungal-specific motif of MtCLR-2 was found to be strongly involved in cellulase secretion, conidium formation, hyphal branching, and colony formation. Mutation of the fungus-specific motif caused significant defects in these characteristics. Thus, we developed an efficient thermophilic fungus-compatible base-editing system that could also be used for genetic engineering in other relevant filamentous fungi.

IMPORTANCE A CRISPR/Cas-based base-editing approach has been developed to introduce point mutations without inducing double-strand breaks (DSBs) and attracted substantial academic and industrial interest. Our study developed the deaminase-cytosine base-editing system to efficiently edit three target genes, amdS, cre-1, and the essential cellulase regulator gene Mtclr-2, in Myceliophthora thermophila. A variety of point mutations in the target loci of the DNA-binding domain and fungus-specific motif of M. thermophila CLR-2 (MtCLR-2) were successfully generated via our base editor Mtevo-CDA1 to elucidate its function. Here, we show that the DNA-binding domain of MtCLR-2 is important for the fungal response to cellulose conditions, while its fungus-specific motif is involved in fungal growth. These findings indicate that our base editor can be an effective tool for elucidating the functions of motifs of target genes in filamentous fungi and for metabolic engineering in the field of synthetic biology.

CRISPR/Cas9-Based Genome Editing and Its Application in Aspergillus Species

Aspergillus, a genus of filamentous fungi, is extensively distributed in nature and plays crucial roles in the decomposition of organic materials as an important environmental microorganism as well as in the traditional fermentation and food processing industries. Furthermore, due to their strong potential to secrete a large variety of hydrolytic enzymes and other natural products by manipulating gene expression and/or introducing new biosynthetic pathways, several Aspergillus species have been widely exploited as microbial cell factories. In recent years, with the development of next-generation genome sequencing technology and genetic engineering methods, the production and utilization of various homo-/heterologous-proteins and natural products in Aspergillus species have been well studied. As a newly developed genome editing technology, the clustered regularly interspaced short palindromic repeats/CRISPR-associated protein 9 (CRISPR/Cas9) system has been used to edit and modify genes in Aspergilli. So far, the CRISPR/Cas9-based approach has been widely employed to improve the efficiency of gene modification in the strain type Aspergillus nidulans and other industrially important and pathogenic Aspergillus species, including Aspergillus oryzae, Aspergillus niger, and Aspergillus fumigatus. This review highlights the current development of CRISPR/Cas9-based genome editing technology and its application in basic research and the production of recombination proteins and natural products in the Aspergillus species.

Marker-free CRISPR-Cas9 based genetic engineering of the phytopathogenic fungus, Penicillium expansum

Filamentous fungi are prolific producers of secondary metabolites (SecMets), including compounds with antibiotic properties, like penicillin, that allows the producing fungus to combat competitors in a shared niche. However, the biological function of the majority of these small complex metabolites for the producing fungi remains unclear (Macheleidt et al., 2016). In an effort to address this lack of knowledge, we have chosen to study the microbial community of moldy apples in the hope of shedding more light on the role of SecMets for the dynamics of the microbial community. Penicillium expansum is one of the prevalent fungal species in this system, and in co-culture experiments with other apple fungal pathogens, we have observed up- and downregulation of several SecMets when compared to monocultures. However, molecular genetic dissection of the observed changes is challenging, and new methodologies for targeted genetic engineering in P. expansum are needed. In the current study, we have established a CRISPR-Cas9 dependent genetic engineering toolbox for the targeted genetic manipulation of P. expansum to allow for single-step construction of marker-free strains. The method and effect of different combinations of a Cas9-sgRNA expressing plasmids and repair template substrates in the NHEJ-proficient WT strain is tested by targeted deletion of melA, encoding a PKS responsible for pigment formation, which upon deletion resulted in white mutants. Co-transformation with a linear double-stranded DNA fragment consisting of two 2 kb homology arms flanking the PKS gene proved to be the most efficient strategy with 100% confirmed deletions by diagnostic PCR. Shorter homology arms (500-1000bp) resulted in 20-30% deletion efficiency. Furthermore, we demonstrate the application of the CRISPR-Cas9 method for targeted deletion of biosynthetic genes without a visible phenotype, insertion of a visual reporter-encoding gene (mRFP), and overexpression of biosynthetic genes. Combined, these tools will advance in enabling the deciphering of SecMet biosynthetic pathways, provide in situ insight into when and where SecMets are produced, and provide an avenue to study the role of P. expansum SecMets in shaping the microbial community development on moldy apples via marker-free targeted genetic engineering of P. expansum.

Application of recyclable CRISPR/Cas9 tools for targeted genome editing in the postharvest pathogenic fungi Penicillium digitatum and Penicillium expansum

Penicillium digitatum and Penicillium expansum are plant pathogenic fungi that cause the green and blue mold diseases, respectively, leading to serious postharvest economic losses worldwide. Moreover, P. expansum can produce mycotoxins, which are hazardous compounds to human and animal health. The development of tools that allow multiple and precise genetic manipulation of these species is crucial for the functional characterization of their genes. In this sense, CRISPR/Cas9 represents an excellent opportunity for genome editing due to its efficiency, accuracy and versatility. In this study, we developed protoplast generation and transformation protocols and applied them to implement the CRISPR/Cas9 technology in both species for the first time. For this, we used a self-replicative, recyclable AMA1-based plasmid which allows unlimited number of genomic modifications without the limitation of integrative selection markers. As test case, we successfully targeted the wetA gene, which encodes a regulator of conidiophore development. Finally, CRISPR/Cas9-derived ΔwetA strains were analyzed. Mutants showed reduced axenic growth, differential pathogenicity and altered conidiogenesis and germination. Additionally, P. digitatum and P. expansum ΔwetA mutants showed distinct sensitivity to fungal antifungal proteins (AFPs), which are small, cationic, cysteine-rich proteins that have become interesting antifungals to be applied in agriculture, medicine and in the food industry. With this work, we demonstrate the feasibility of the CRISPR/Cas9 system, expanding the repertoire of genetic engineering tools available for these two important postharvest pathogens and open up the possibility to adapt them to other economically relevant phytopathogenic fungi, for which toolkits for genetic modifications are often limited.

Fungal Proteases as Emerging Biocatalysts to Meet the Current Challenges and Recent Developments in Biomedical Therapies: An Updated Review

With the increasing world population, demand for industrialization has also increased to fulfill humans' living standards. Fungi are considered a source of essential constituents to produce the biocatalytic enzymes, including amylases, proteases, lipases, and cellulases that contain broad-spectrum industrial and emerging applications. The present review discussed the origin, nature, mechanism of action, emerging aspects of genetic engineering for designing novel proteases, genome editing of fungal strains through CRISPR technology, present challenges and future recommendations of fungal proteases. The emerging evidence revealed that fungal proteases show a protective role to many environmental exposures and discovered that an imbalance of protease inhibitors and proteases in the epithelial barriers leads to the protection of chronic eosinophilic airway inflammation. Moreover, mitoproteases recently were found to execute intense proteolytic processes that are crucial for mitochondrial integrity and homeostasis function, including mitochondrial biogenesis, protein synthesis, and apoptosis. The emerging evidence revealed that CRISPR/Cas9 technology had been successfully developed in various filamentous fungi and higher fungi for editing of specific genes. In addition to medical importance, fungal proteases are extensively used in different industries such as foods to prepare butter, fruits, juices, and cheese, and to increase their shelf life. It is concluded that hydrolysis of proteins in industries is one of the most significant applications of fungal enzymes that led to massive usage of proteomics.

Engineering interventions in industrial filamentous fungal cell factories for biomass valorization

Filamentous fungi possess versatile capabilities for synthesizing a variety of valuable bio compounds, including enzymes, organic acids and small molecule secondary metabolites. The advancements of genetic and metabolic engineering techniques and the availability of sequenced genomes discovered their potential as expression hosts for recombinant protein production. Remarkably, plant-biomass degrading filamentous fungi show the unique capability to decompose lignocellulose, an extremely recalcitrant biopolymer. The basic biochemical approaches have motivated several industrial processes for lignocellulose biomass valorisation into fermentable sugars and other biochemical for biofuels, biomolecules, and biomaterials. The review gives insight into current trends in engineering filamentous fungi for enzymes, fuels, and chemicals from lignocellulose biomass. This review describes the variety of enzymes and compounds that filamentous fungi produce, engineering of filamentous fungi for biomass valorisation with a special focus on lignocellulolytic enzymes and other bulk chemicals.

Evidence of the Involvement of a Cyclase Gene in the Biosynthesis of Ochratoxin A in Aspergillus carbonarius

Ochratoxin A (OTA) is a well-known mycotoxin with wide distribution in food and feed. Fungal genome sequencing has great utility for identifying secondary metabolites gene clusters for known and novel compounds. A comparative analysis of the OTA-biosynthetic cluster in A. steynii, A. westerdijkiae, A. niger, A. carbonarius, and P. nordicum has revealed a high synteny in OTA cluster organization in five structural genes (otaA, otaB, ota, otaR1, and otaD). Moreover, a recent detailed comparative genome analysis of Aspergilli OTA producers led to the identification of a cyclase gene, otaY, located in the OTA cluster between the otaA and otaB genes, encoding for a predicted protein with high similarity to SnoaLs domain. These proteins have been shown to catalyze ring closure steps in the biosynthesis of polyketide antibiotics produced in Streptomyces. In the present study, we demonstrated an upregulation of the cyclase gene in A. carbonarius under OTA permissive conditions, consistent with the expression trends of the other OTA cluster genes and their role in OTA biosynthesis by complete gene deletion. Our results pointed out the involvement of a cyclase gene in OTA biosynthetic pathway for the first time. They represent a step forward in the understanding of the molecular basis of OTA biosynthesis in A. carbonarius.

Recent Molecular Tools for the Genetic Manipulation of Highly Industrially Important Mucoromycota Fungi

Mucorales is the largest and most well-studied order of the phylum Mucormycota and is known for its rapid growth rate and various industrial applications. The Mucorales fungi are a fascinating group of filamentous organisms with many uses in research and the industrial and medical fields. They are widely used biotechnological producers of various secondary metabolites and other value-added products. Certain members of Mucorales are extensively used as model organisms for genetic and molecular investigation and have extended our understanding of the metabolisms of other members of this order as well. Compared with other fungal species, our understanding of Mucoralean fungi is still in its infancy, which could be linked to their lack of effective genetic tools. However, recent advancements in molecular tools and approaches, such as the construction of recyclable markers, silencing vectors, and the CRISPR-Cas9-based gene-editing system, have helped us to modify the genomes of these model organisms. Multiple genetic modifications have been shown to generate valuable products on a large scale and helped us to understand the morphogenesis, basic biology, pathogenesis, and host–pathogen interactions of Mucoralean fungi. In this review, we discuss various conventional and modern genetic tools and approaches used for efficient gene modification in industrially important members of Mucorales.

An electrochemical protocol for CRISPR-mediated gene-editing of sheep embryonic fibroblast cells

Genetic engineering of farm animals is commonly carried out via cell-mediated transfection followed by somatic cell nuclear transfer. However, efficient transfer of exogenous DNA into ovine embryonic fibroblast (EF) cells without compromising cell viability have remained a challenging issue. Here, we aimed to develop a protocol for electrotransfection of sheep EF cells. First, we optimized the pulsing condition using an OptiMEM-GlutaMAX medium as the electroporation buffer and found two pulses of 270 V, each for 10 ms and 10 s interval, is the most efficient condition to have a high rate of transfection and cell survival. Moreover, supplementing 3 % dimethyl sulfoxide (DMSO) into the electroporation medium considerably improved the cell viability after the electroporation process. The electroporation procedure resulted in > 98% transfection efficiency and > 97 % cell survival rate using reporter plasmids. Finally, using CRISPR/Cas9-encoding vectors, we targeted BMP15 and GDF9 genes in sheep EF cells. The electroporated cells are associated with a 52 % indels rate using single gRNAs as well as a highly efficient target deletion using two gRNAs. In conclusion, we developed an electrotransfection protocol using the OptiMEM-GlutaMAX medium supplemented with 3 % DMSO for sheep EF cells. The electroporation method can be used for cell-mediated gene-editing in sheep.

The important role of P450 monooxygenase for the biosynthesis of new benzophenones from Cytospora rhizophorae

Benzophenones are polyketides with diverse biological activities. Novel cytotoxic benzophenones cytosporaphenones A-C and cytorhizins A-D, which contain a new skeleton, were previously extracted from endophytic fungus Cytospora rhizophorae A761. However, the mechanism for the biosynthesis of these compounds remains unknown. Cytosporaphenone A was assumed to be the precursor for the biosynthesis of cytorhizins A-D. In this study, we sequenced the genome of C. rhizophorae A761 and characterized a benzoate 4-monooxygenase cytochrome P450(BAM). CRISPR/Cas9-mediated gene knockout and overexpression studies in C. rhizophorae confirmed the vital function of BAM in the biosynthesis of cytosporaphenones and cytorhizins. Overexpression of BAM also enhanced the yield of cytosporaphenone A by 1.868 folds. The in vitro function and enzymatic properties of BAM were also described. This study demonstrates the important role of BAM for the biosynthesis of cytosporaphenone A and cytorhizins and is also the first to provide approaches for the CRISPR-Cas9-mediated gene deletion and gene overexpression studies in C. rhizophoarae, thus laying a foundation for the elucidation of the biosynthetic mechanism of cytorhizins and the discovery of new benzophenones mediated by BAM.Key points• The novel bam gene encoding BAM protein in C. rhizophorae was firstly deleted using CRIPSR/Cas9 system.• The in vitro oxidation function of novel BAM protein and enzymatic properties was characterized.• The over expression of bam gene enhanced the yield of cytosporaphone A in C. rhizophorae significantly.

CRISPR/Cas9 mediated editing of the Quorn fungus Fusarium venenatum A3/5 by transient expression of Cas9 and sgRNAs targeting endogenous marker gene PKS12

Background

Gene editing using CRISPR/Cas9 is a widely used tool for precise gene modification, modulating gene expression and introducing novel proteins, and its use has been reported in various filamentous fungi including the genus Fusarium. The aim of this study was to optimise gene editing efficiency using AMA1 replicator vectors for transient expression of CRISPR constituents in Fusarium venenatum (A3/5), used commercially in the production of mycoprotein (Quorn™).

Results

We present evidence of CRISPR/Cas9 mediated gene editing in Fusarium venenatum, by targeting the endogenous visible marker gene PKS12, which encodes a polyketide synthase responsible for the synthesis of the pigment aurofusarin. Constructs for expression of single guide RNAs (sgRNAs) were cloned into an AMA1 replicator vector incorporating a construct for constitutive expression of cas9 codon-optimised for Aspergillus niger or F. venenatum. Vectors were maintained under selection for transient expression of sgRNAs and cas9 in transformed protoplasts. 100% gene editing efficiency of protoplast-derived isolates was obtained using A. niger cas9 when sgRNA transcription was regulated by the F. venenatum 5SrRNA promoter. In comparison, expression of sgRNAs using a PgdpA-ribozyme construct was much less effective, generating mutant phenotypes in 0–40% of isolates. Viable isolates were not obtained from protoplasts transformed with an AMA1 vector expressing cas9 codon-optimised for F. venenatum.

Conclusions

Using an AMA1 replicator vector for transient expression of A. niger cas9 and sgRNAs transcribed from the native 5SrRNA promoter, we demonstrate efficient gene editing of an endogenous marker gene in F. venenatum, resulting in knockout of gene function and a visible mutant phenotype in 100% of isolates. This establishes a platform for further development of CRISPR/Cas technology in F. venenatum for use as a research tool, for understanding the controls of secondary metabolism and hyphal development and validating prototypes of strains produced using traditional methods for strain improvement.

Supplementary Information

The online version contains supplementary material available at 10.1186/s40694-021-00121-8.

Efficient genome editing in filamentous fungi via an improved CRISPR-Cas9 ribonucleoprotein method facilitated by chemical reagents

DNA double-strand break (DSB) repair induced by the RNA-programmed nuclease Cas9 has become a popular method for genome editing. Direct genome editing via Cas9-CRISPR gRNA (guide RNA) ribonucleoprotein (RNP) complexes assembled in vitro has also been successful in some fungi. However, the efficiency of direct RNP transformation into fungal protoplasts is currently too low. Here, we report an optimized genome editing approach for filamentous fungi based on RNPs facilitated by adding chemical reagents. We increased the transformation efficiency of RNPs significantly by adding Triton X-100 and prolonging the incubation time, and the editing efficiency reached 100% in Trichoderma reesei and Cordyceps militaris. The optimized RNP-based method also achieved efficient (56.52%) homologous recombination integration with short homology arms (20 bp) and gene disruption (7.37%) that excludes any foreign DNA (selection marker) in T. reesei. In particular, after adding reagents related to mitosis and cell division, the further optimized protocol showed an increased ratio of edited homokaryotic transformants (from 0% to 40.0% for inositol and 71.43% for benomyl) from Aspergillus oryzae, which contains multinucleate spores and protoplasts. Furthermore, the multi-target engineering efficiency of the optimized RNP transformation method was similar to those of methods based on in vivo expression of Cas9. This newly established genome editing system based on RNPs may be widely applicable to construction of genome-edited fungi for the food and medical industries, and has good prospects for commercialization.

CRISPR/Cas9-mediated genome editing directed by a 5S rRNA-tRNAGly hybrid promoter in the thermophilic filamentous fungus Humicola insolens

BACKGROUND

Humicola insolens is a filamentous fungus with high potential of producing neutral and heat- and alkali-resistant cellulase. However, the genetic engineering tools, particularly the genome-editing tool, are scarce, hindering the study of cellulase expression regulation in this organism.

RESULTS

Herein, a CRISPR/Cas9 genome-editing system was established in H. insolens based on a hybrid 5S rRNA-tRNA^Gly promoter. This system is superior to the HDV (hepatitis delta virus) system in genome editing, allowing highly efficient single gene destruction in H. insolens with rates of deletion up to 84.1% (37/44). With this system, a putative pigment synthesis gene pks and the transcription factor xyr1 gene were disrupted with high efficiency. Moreover, the extracellular protein concentration and cellulase activity largely decreased when xyr1 was deleted, demonstrating for the first time that Xyr1 plays an important role in cellulase expression regulation.

CONCLUSIONS

The established CRISPR/Cas9 system is a powerful genetic operation tool for H. insolens, which will accelerate studies on the regulation mechanism of cellulase expression and engineering of H. insolens for higher cellulase production.

Application of CRISPR/Cas9 Tools for Genome Editing in the White-Rot Fungus Dichomitus squalens

Dichomitus squalens is an emerging reference species that can be used to investigate white-rot fungal plant biomass degradation, as it has flexible physiology to utilize different types of biomass as sources of carbon and energy. Recent comparative (post-) genomic studies on D. squalens resulted in an increasingly detailed knowledge of the genes and enzymes involved in the lignocellulose breakdown in this fungus and showed a complex transcriptional response in the presence of lignocellulose-derived compounds. To fully utilize this increasing amount of data, efficient and reliable genetic manipulation tools are needed, e.g., to characterize the function of certain proteins in vivo and facilitate the construction of strains with enhanced lignocellulolytic capabilities. However, precise genome alterations are often very difficult in wild-type basidiomycetes partially due to extremely low frequencies of homology directed recombination (HDR) and limited availability of selectable markers. To overcome these obstacles, we assessed various Cas9-single guide RNA (sgRNA) ribonucleoprotein (RNP) -based strategies for selectable homology and non-homologous end joining (NHEJ) -based gene editing in D. squalens. We also showed an induction of HDR-based genetic modifications by using single-stranded oligodeoxynucleotides (ssODNs) in a basidiomycete fungus for the first time. This paper provides directions for the application of targeted CRISPR/Cas9-based genome editing in D. squalens and other wild-type (basidiomycete) fungi.

Plant and Fungal Genome Editing to Enhance Plant Disease Resistance Using the CRISPR/Cas9 System

Crop production has been substantially reduced by devastating fungal and oomycete pathogens, and these pathogens continue to threaten global food security. Although chemical and cultural controls have been used for crop protection, these involve continuous costs and time and fungicide resistance among plant pathogens has been increasingly reported. The most efficient way to protect crops from plant pathogens is cultivation of disease-resistant cultivars. However, traditional breeding approaches are laborious and time intensive. Recently, the CRISPR/Cas9 system has been utilized to enhance disease resistance among different crops such as rice, cacao, wheat, tomato, and grape. This system allows for precise genome editing of various organisms via RNA-guided DNA endonuclease activity. Beyond genome editing in crops, editing the genomes of fungal and oomycete pathogens can also provide new strategies for plant disease management. This review focuses on the recent studies of plant disease resistance against fungal and oomycete pathogens using the CRISPR/Cas9 system. For long-term plant disease management, the targeting of multiple plant disease resistance mechanisms with CRISPR/Cas9 and insights gained by probing fungal and oomycete genomes with this system will be powerful approaches.

Tailoring in fungi for next generation cellulase production with special reference to CRISPR/CAS system

Cellulose is the utmost plenteous source of biopolymer in our earth, and fungi are the most efficient and ubiquitous organism in degrading the cellulosic biomass by synthesizing cellulases. Tailoring through genetic manipulation has played a substantial role in constructing novel fungal strains towards improved cellulase production of desired traits. However, the traditional methods of genetic manipulation of fungi are time-consuming and tedious. With the availability of the full-genome sequences of several industrially relevant filamentous fungi, CRISPR-CAS (clustered regularly interspaced short palindromic repeats/CRISPR-associated protein) technology has come into the focus for the proficient development of manipulated strains of filamentous fungi. This review summarizes the mode of action of cellulases, transcription level regulation for cellulase expression, various traditional strategies of genetic manipulation with CRISPR-CAS technology to develop modified fungal strains for a preferred level of cellulase production, and the futuristic trend in this arena of research.