Rate Of Homologous Recombination Research Articles

Measuring Homologous Recombination Rates between Chromosomal Locations in Salmonella.

Homologous recombination between two similar DNA molecules, plays an important role in the repair of double-stranded DNA breaks. Recombination can occur between two sister chromosomes, or between two locations of similar sequence identity within the same chromosome. The assay described here is designed to measure the rate of homologous recombination between two locations with sequence similarity within the same bacterial chromosome. For this purpose, a selectable/counter-selectable genetic cassette is inserted into one of the locations and homologous recombination repair rates are measured as a function of recombinational removal of the inserted cassette. This recombinational repair process is called gene conversion, non-reciprocal recombination. We used this method to measure the recombination rates between genes within gene families and to study the stability of mobile genetic elements inserted into members of gene families.

Genetic exchanges are more frequent in bacteria encoding capsules.

Capsules allow bacteria to colonize novel environments, to withstand numerous stresses, and to resist antibiotics. Yet, even though genetic exchanges with other cells should be adaptive under such circumstances, it has been suggested that capsules lower the rates of homologous recombination and horizontal gene transfer. We analysed over one hundred pan-genomes and thousands of bacterial genomes for the evidence of an association between genetic exchanges (or lack thereof) and the presence of a capsule system. We found that bacteria encoding capsules have larger pan-genomes, higher rates of horizontal gene transfer, and higher rates of homologous recombination in their core genomes. Accordingly, genomes encoding capsules have more plasmids, conjugative elements, transposases, prophages, and integrons. Furthermore, capsular loci are frequent in plasmids, and can be found in prophages. These results are valid for Bacteria, independently of their ability to be naturally transformable. Since we have shown previously that capsules are commonly present in nosocomial pathogens, we analysed their co-occurrence with antibiotic resistance genes. Genomes encoding capsules have more antibiotic resistance genes, especially those encoding efflux pumps, and they constitute the majority of the most worrisome nosocomial bacteria. We conclude that bacteria with capsule systems are more genetically diverse and have fast-evolving gene repertoires, which may further contribute to their success in colonizing novel niches such as humans under antibiotic therapy.

A Single -195 C < G HBG1 Promoter Mediated By CRISPR/Cas9 Genome Editing Induces Fetal Hemoglobin Synthesis in Hudep-2

Sickle cell disease (SCD) is a serious condition, chronic and undoubtedly represents a public health problem worldwide. SCD is caused by a point mutation in codon 6 of the β globin gene resulting in the production of a structurally abnormal hemoglobin, hemoglobin S. Although the cause of the disease has been known for more than fifty years, therapeutic options are still quite limited.High levels of fetal hemoglobin (HbF) in the blood are associated with a better clinical outcome in SCD patients. In some individuals, the expression of γ-globin gene persists into adulthood in elevated levels, which is called hereditary persistence of fetal hemoglobin (HPFH). A single nucleotide mutation from C to G at position -195 of the HBG1 gene promoter, called non deletional HPFH Brazilian type (nd-HPFH-B), augments the levels of HbF in patients in 7%- 30%. Nd-HPFH-B has been described by our group, but the mechanism and how this single mutation rises HbF levels differently in red blood cells is still unknown. Genome editing using CRISPR/Cas9 in HUDEP-2 cell, an erythroid precursor line, has been developed through homologous direct repair from a small single DNA strand containing the guanine in -195 position at HBG1 gene promotor. All the other genes, including the second HBG1 allele were unaltered.This point mutation has been carried out by CRISPR/Cas9 high fidelity system, capable of performing a specific break in the DNA target sequence, that improves homologous recombination rate of the donor sequence containing the -195 C<G mutation (ssODN -195).For the first time, we generated a HUDEP-2 cell line with the -195 C>T mutation in HBG1 promoter using CRISPR/Cas9 genome editing. The HUDEP-2 cells were nucleofected with Cas9 high fidelity ribonucleoprotein (104 pmol), crRNA:tracrRNA (120 pmol) complex and 1uM ssODN -195, using CD34+ human cell kit and program E-001 in AMAXA Nucleofector 4D- device (Lonza). Seven days after nucleofection, the transformed cells were submitted to clonal selection for 25 days. The genomic DNA from 48 clones were submitted by Sanger Sequencing. The sequencing analysis showed highest Crispr/Cas9 efficiency in genomic DNA cut (77.08%; 37/48) and satisfactory ssODN -195 homologous recombination (10.4%; 5/48).Five nd-HPFH-B HUDEP-2 clones and three other clones without the mutation, but with indels after Cas9 DNA cut (controls), were expanded in culture and the HbF levels were measure with anti-HbF antibody by flow cytometry in two biological replicates. HbF levels in nd-HPFH-B HUDEP-2 clones were 6.02%±1.4, 8.25% ± 0.28, 10.18% ± 3.71, 11.95% ± 0.49, 26,3% ± 4,6 while in controls were 1.69% ± 0.26, 1.66% ± 0.26, 0.59% ± 0.06. Two nd-HPFH-B clones were differentiated into erythrocyte in vitro, and fetal hemoglobin levels persisted at high levels seen previously.In addition, α-globin, β-globin and γ-globin mRNA levels were evaluated in three nd-HPFH-B HUDEP-2 clones and two control clones. The mRNA HBG1/HBG1+HBB percentage in nd-HPFH-B were 96.16% ± 4.10 against 22.63% ± 9.64 in controls.The monoallelic single nucleotide mutation -195 C>G is capable to increase the fetal hemoglobin levels up to 30% in nd-HPFH-B HUDEP-2, and our results shows that this is a potential experimental in vitro model to be used in future studies. DisclosuresNo relevant conflicts of interest to declare.

Deletion of VdKu80 enhances targeted gene replacement in Verticillium dahliae

Verticillium dahliae is a notorious phytopathogenic fungus and causes severe Verticillium wilt diseases worldwide. The available genomic sequence of V. dahliae has facilitated genome-wide investigation of its life cycle and disease process. However, inefficient targeted gene replacement hampers gene functional analysis of V. dahliae. Ku heterodimer genes Ku70 and Ku80 have been proved to be involved in the recognition of DNA double-strand breaks, which will reduce the rate of homologous recombination. Here, in order to improve the frequency of the homologous recombination, we identified and deleted the V. dahliae VdKu80 with bioinformatics methods and protoplast-mediated transformation, respectively. The phenotypes of VdKu80 deletion mutants, such as fungal growth, microsclerotia formation and virulence, were similar to those of the wild type strain. Remarkably, the gene replacement frequencies of two genes (VDAG_00736 and VDAG_07169 which encode the cell division control protein) were increased by about 20% with VdKu80 deletion mutant as a recipient strain compared with that of the wild type strain. The results suggest that deletion of VdKu80 triggered the enhancement of the gene replacement frequency, indicating that the ∆VdKu80 strain can be used as an efficient recipient for the targeted gene manipulation in V. dahliae.

CRISPR-Cas9 genome editing induces a p53-mediated DNA damage response.

Here, we report that genome editing by CRISPR-Cas9 induces a p53-mediated DNA damage response and cell cycle arrest in immortalized human retinal pigment epithelial cells, leading to a selection against cells with a functional p53 pathway. Inhibition of p53 prevents the damage response and increases the rate of homologous recombination from a donor template. These results suggest that p53 inhibition may improve the efficiency of genome editing of untransformed cells and that p53 function should be monitored when developing cell-based therapies utilizing CRISPR-Cas9.

A Simple and Universal System for Gene Manipulation in Aspergillus fumigatus: In Vitro-Assembled Cas9-Guide RNA Ribonucleoproteins Coupled with Microhomology Repair Templates.

CRISPR (clustered regularly interspaced short palindromic repeat)-Cas9 is a novel genome-editing system that has been successfully established in Aspergillus fumigatus. However, the current state of the technology relies heavily on DNA-based expression cassettes for delivering Cas9 and the guide RNA (gRNA) to the cell. Therefore, the power of the technology is limited to strains that are engineered to express Cas9 and gRNA. To overcome such limitations, we developed a simple and universal CRISPR-Cas9 system for gene deletion that works across different genetic backgrounds of A.fumigatus. The system employs in vitro assembly of dual Cas9 ribonucleoproteins (RNPs) for targeted gene deletion. Additionally, our CRISPR-Cas9 system utilizes 35 to 50bp of flanking regions for mediating homologous recombination at Cas9 double-strand breaks (DSBs). As a proof of concept, we first tested our system in the ΔakuB (ΔakuBku80 ) laboratory strain and generated high rates (97%) of gene deletion using 2µg of the repair template flanked by homology regions as short as 35bp. Next, we inspected the portability of our system across other genetic backgrounds of A.fumigatus, namely, the wild-type strain Af293 and a clinical isolate, A.fumigatus DI15-102. In the Af293 strain, 2µg of the repair template flanked by 35 and 50bp of homology resulted in highly efficient gene deletion (46% and 74%, respectively) in comparison to classical gene replacement systems. Similar deletion efficiencies were also obtained in the clinical isolate DI15-102. Taken together, our data show that in vitro-assembled Cas9 RNPs coupled with microhomology repair templates are an efficient and universal system for gene manipulation in A.fumigatus. IMPORTANCE Tackling the multifactorial nature of virulence and antifungal drug resistance in A.fumigatus requires the mechanistic interrogation of a multitude of genes, sometimes across multiple genetic backgrounds. Classical fungal gene replacement systems can be laborious and time-consuming and, in wild-type isolates, are impeded by low rates of homologous recombination. Our simple and universal CRISPR-Cas9 system for gene manipulation generates efficient gene targeting across different genetic backgrounds of A.fumigatus. We anticipate that our system will simplify genome editing in A.fumigatus, allowing for the generation of single- and multigene knockout libraries. In addition, our system will facilitate the delineation of virulence factors and antifungal drug resistance genes in different genetic backgrounds of A.fumigatus.

Abstract 3470: The promyelocytic leukemia (PML) protein modulates rate and localization of homologous recombination in human cell lines with the alternative lengthening of telomeres (ALT) pathway

Abstract The promyelocytic leukemia protein (PML) is tightly associated with a defining feature of the cancer specific, telomerase-independent telomere-maintenance pathway known as alternative lengthening of telomeres (ALT); therefore, PML is an important potential target for chemotherapeutics. Cells running ALT contain large accumulations of telomeric DNA and RNA in the nucleoplasm that are frequently coated in a polymer shell of PML protein. These structures are known as ALT-associated PML bodies (APBs). APBs have been postulated to be major sites of the telomeric sequence homologous recombination believed to be the basis of telomere maintenance in ALT. A CRISPR based strategy was used to knock out the PML gene in two widely used ALT positive osteosarcoma-derived human cell lines; U2OS, and SAOS2. Knockout clones from both cell lines continued to proliferate past passage 90 without crisis, and knockouts were validated at the genetic and protein levels by Sanger sequencing and western blotting, respectively. Chromosome orientation fluorescent in situ hybridization (COFISH) was carried out to determine the number of telomere sequence exchanges occurring in a single cell cycle in these knockouts. A twofold increase in telomere-specific exchanges, presumably telomere sister chromatid exchanges (T-SCE), over the parental line was detected. Intrachromosomal exchanges not specific to telomeres were also analyzed by the harlequin chromosome staining method. A significant increase in these types of exchanges was also observed. In conclusion, the presence of PML is not required for ALT to continue to function, and may be acting to modulate homologous recombination frequency and location in ALT positive cells. Citation Format: Walter Barry, Christopher Heaphy, Alan Meeker. The promyelocytic leukemia (PML) protein modulates rate and localization of homologous recombination in human cell lines with the alternative lengthening of telomeres (ALT) pathway [abstract]. In: Proceedings of the American Association for Cancer Research Annual Meeting 2017; 2017 Apr 1-5; Washington, DC. Philadelphia (PA): AACR; Cancer Res 2017;77(13 Suppl):Abstract nr 3470. doi:10.1158/1538-7445.AM2017-3470

Prokaryote genome fluidity is dependent on effective population size

Many prokaryote species are known to have fluid genomes, with different strains varying markedly in accessory gene content through the combined action of gene loss, gene gain via lateral transfer, as well as gene duplication. However, the evolutionary forces determining genome fluidity are not yet well understood. We here for the first time systematically analyse the degree to which this distinctive genomic feature differs between bacterial species. We find that genome fluidity is positively correlated with synonymous nucleotide diversity of the core genome, a measure of effective population size Ne. No effects of genome size, phylogeny or homologous recombination rate on genome fluidity were found. Our findings are consistent with a scenario where accessory gene content turnover is for a large part dictated by neutral evolution.

CRISPR/Cas9-mediated efficient genome editing via blastospore-based transformation in entomopathogenic fungus Beauveria bassiana

Beauveria bassiana is an environmentally friendly alternative to chemical insecticides against various agricultural insect pests and vectors of human diseases. However, its application has been limited due to slow kill and sensitivity to abiotic stresses. Understanding of the molecular pathogenesis and physiological characteristics would facilitate improvement of the fungal performance. Loss-of-function mutagenesis is the most powerful tool to characterize gene functions, but it is hampered by the low rate of homologous recombination and the limited availability of selectable markers. Here, by combining the use of uridine auxotrophy as recipient and donor DNAs harboring auxotrophic complementation gene ura5 as a selectable marker with the blastospore-based transformation system, we established a highly efficient, low false-positive background and cost-effective CRISPR/Cas9-mediated gene editing system in B. bassiana. This system has been demonstrated as a simple and powerful tool for targeted gene knock-out and/or knock-in in B. bassiana in a single gene disruption. We further demonstrated that our system allows simultaneous disruption of multiple genes via homology-directed repair in a single transformation. This technology will allow us to study functionally redundant genes and holds significant potential to greatly accelerate functional genomics studies of B. bassiana.

Correlated Mutations and Homologous Recombination Within Bacterial Populations.

Inferring the rate of homologous recombination within a bacterial population remains a key challenge in quantifying the basic parameters of bacterial evolution. Due to the high sequence similarity within a clonal population, and unique aspects of bacterial DNA transfer processes, detecting recombination events based on phylogenetic reconstruction is often difficult, and estimating recombination rates using coalescent model-based methods is computationally expensive, and often infeasible for large sequencing data sets. Here, we present an efficient solution by introducing a set of mutational correlation functions computed using pairwise sequence comparison, which characterize various facets of bacterial recombination. We provide analytical expressions for these functions, which precisely recapitulate simulation results of neutral and adapting populations under different coalescent models. We used these to fit correlation functions measured at synonymous substitutions using whole-genome data on Escherichia coli and Streptococcus pneumoniae populations. We calculated and corrected for the effect of sample selection bias, i.e., the uneven sampling of individuals from natural microbial populations that exists in most datasets. Our method is fast and efficient, and does not employ phylogenetic inference or other computationally intensive numerics. By simply fitting analytical forms to measurements from sequence data, we show that recombination rates can be inferred, and the relative ages of different samples can be estimated. Our approach, which is based on population genetic modeling, is broadly applicable to a wide variety of data, and its computational efficiency makes it particularly attractive for use in the analysis of large sequencing datasets.

Efficient Genome Editing in the Oomycete Phytophthora sojae Using CRISPR/Cas9.

Phytophthora is a filamentous fungus-like microorganism, but belongs to the oomycetes, in the kingdom Stramenopila. Phytophthora species are notorious as plant destroyers, causing multibillion-dollar damage to agriculture and natural ecosystems worldwide annually. For a long time, genome editing has been unattainable in oomycetes, because of their extremely low rate of homologous recombination. The recent implementation of the CRISPR/Cas (clustered regularly interspaced short palindromic repeats/CRISPR-associated) system in the soybean pathogen Phytophthora sojae, an experimental model for oomycetes, has opened up a powerful new research capability for the oomycete community. Here, we describe a detailed protocol for CRISPR/Cas9-mediated genome editing in P. sojae, including single guide RNA (sgRNA) design and construction, efficient gene replacement, and mutant-screening strategies. This protocol should be generally applicable for most culturable oomycetes. We also describe an optimized transformation method that is useful for other Phytophthora spp. including P. capsici and P. parasitica. © 2017 by John Wiley & Sons, Inc.

Molecular diversity of Wolbachia in Lepidoptera: Prevalent allelic content and high recombination of MLST genes

Wolbachia are common endosymbiotic bacteria of Arthropoda and Nematoda that are ordinarily transmitted vertically in host lineages through the egg cytoplasm. Despite the great interest in the Wolbachia symbiont, many issues of its biology remain unclear, including its evolutionary history, routes of transfer among species, and the molecular mechanisms underlying the symbiont's effect on its host. In this report, we present data relating to Wolbachia infection in 120 species of 13 Lepidoptera families, mostly butterflies, from West Siberian localities based on Multilocus sequence typing (MLST) and the wsp locus and perform a comprehensive survey of the distribution of Wolbachia and its genetic diversity in Lepidoptera worldwide. We observed a high infection incidence in the studied region; this finding is probably also true for other temperate latitude regions because many studied species have broad Palearctic and even Holarctic distribution. Although 40 new MLST alleles and 31 new STs were described, there was no noticeable difference in the MLST allele content in butterflies and probably also in moths worldwide. A genetic analysis of Wolbachia strains revealed the MLST allele core in lepidopteran hosts worldwide, viz. the ST-41 allele content. The key finding of our study was the detection of rampant recombination among MLST haplotypes. High rates of homologous recombination between Wolbachia strains indicate a substantial contribution of genetic exchanges to the generation of new STs. This finding should be considered when discussing issues related to the reconstruction of Wolbachia evolution, divergence time, and the routes of Wolbachia transmission across arthropod hosts.

Prevalence and genetic diversity of coronaviruses in wild birds, Finland

ABSTRACT Introduction: Migratory birds act as hosts for a number of zoonotic viruses, and have the ability to disperse these viruses to distant geographic locations. Coronaviruses (CoVs) represent a family of zoonotic viruses with wide variety of animal hosts, including birds and humans. The infections caused by coronaviruses vary from mild to severe, depending on the viral species and the host. Since the coronaviruses exhibit extraordinary large RNA genome, also the rate of homologous recombination is high, which in turn contributes to the genetic diversity and interspecies host-switches of CoVs. The emergence of novel CoVs has been rich during the last decades, and wild birds seem to serve as reservoirs for a variety of CoV strains. We examined the CoVs circulating among wild birds in Finland. Materials and methods: Samples (cloacal swab, tracheal swab, oropharyngeal swab, or tissue) representing 61 bird species were collected during 2010-2013, and examined by RT-PCR targeting the RdRp gene for the presence of CoV RNA. Results: Altogether 51/939 (5.4%) of the examined birds were found positive by RT-PCR. Diverse gamma- and deltacoronavirus sequences were detected. Discussion: Gamma- and deltacoronaviruses circulate among wild birds in Finland. The number of CoV-positive birds detected each year varies greatly.

High-efficiency non-mosaic CRISPR-mediated knock-in and indel mutation in F0 Xenopus.

The revolution in CRISPR-mediated genome editing has enabled the mutation and insertion of virtually any DNA sequence, particularly in cell culture where selection can be used to recover relatively rare homologous recombination events. The efficient use of this technology in animal models still presents a number of challenges, including the time to establish mutant lines, mosaic gene editing in founder animals, and low homologous recombination rates. Here we report a method for CRISPR-mediated genome editing in Xenopus oocytes with homology-directed repair (HDR) that provides efficient non-mosaic targeted insertion of small DNA fragments (40-50 nucleotides) in 4.4-25.7% of F0 tadpoles, with germline transmission. For both CRISPR/Cas9-mediated HDR gene editing and indel mutation, the gene-edited F0 embryos are uniformly heterozygous, consistent with a mutation in only the maternal genome. In addition to efficient tagging of proteins in vivo, this HDR methodology will allow researchers to create patient-specific mutations for human disease modeling in Xenopus.

Development of an Improved System for the Generation of Knockout Mutants of Amycolatopsis sp. Strain ATCC 39116.

The Gram-positive actinomycete Amycolatopsis sp. strain ATCC 39116 is used for the industrial production of natural vanillin. Previously, the only gene deletion performed in this strain targeted the gene vdh, coding for a vanillin dehydrogenase. The generation of this mutant suffered from a high number of illegitimate recombinations and a low rate of homologous recombination. To alleviate this, we constructed an optimized deletion system based on a modified suicide vector. Thereby, we were able to increase the rate of homologous integration from less than 1% of the analyzed clones to 20% or 50%, depending on the targeted gene. We were furthermore able to reduce the screening effort needed to identify homogenotes through the use of the rpsL gene from Saccharopolyspora erythraea, which confers streptomycin sensitivity on clones still carrying the suicide vector. The new suicide vector is p6SUI5ERPSL, and its applicability was demonstrated by the deletion of three Amycolatopsis gene clusters. The deletion of the first of the gene clusters, coding for an aldehyde oxidase (yagRST), led to no altered phenotype compared to the parent strain; deletion of the second, coding for a vanillic acid decarboxylase (vdcBCD), led to a phenotype that was strongly impaired in its growth with vanillic acid as the sole carbon source and also unable to form guaiacol; and deletion of the third, coding for a vanillate demethylase (vanAB), led to only a negligible impact in comparison. Therefore, we showed that decarboxylation of vanillic acid is the main degradation pathway in Amycolatopsis sp. ATCC 39116 while the demethylation plays only a minor role and does not compensate the deletion of vdcBCD IMPORTANCE: Amycolatopsis sp. ATCC 39116 is an important microorganism used for the production of natural vanillin from ferulic acid. In contrast to this importance, it has previously been shown that this strain is hard to manipulate on a genetic level. We therefore generated an optimized system to facilitate the deletion of genes in this strain. This allowed us to greatly reduce the time and work requirements for generating deletions. This could allow the improvement of vanillin production in the future and also the elucidation of metabolic pathways. To test our deletion system, we deleted three gene clusters in Amycolatopsis sp. ATCC 39116. One showed no involvement in the metabolism of vanillin, while the second proved to be the main pathway of vanillic acid degradation and completely stopped the formation of the off-flavor guaiacol. The third appeared to have only a negligible impact on the degradation of vanillic acid.

Efficient and versatile CRISPR engineering of human neurons in culture to model neurological disorders.

The recent identification of multiple new genetic causes of neurological disorders highlights the need for model systems that give experimental access to the underlying biology. In particular, the ability to couple disease-causing mutations with human neuronal differentiation systems would be beneficial. Gene targeting is a well-known approach for dissecting gene function, but low rates of homologous recombination in somatic cells (including neuronal cells) have traditionally impeded the development of robust cellular models of neurological disorders. Recently, however, CRISPR/Cas9 gene editing technologies have expanded the number of systems within which gene targeting is possible. Here we adopt as a model system LUHMES cells, a commercially available diploid human female mesencephalic cell line that differentiates into homogeneous mature neurons in 1-2 weeks. We describe optimised methods for transfection and selection of neuronal progenitor cells carrying targeted genomic alterations using CRISPR/Cas9 technology. By targeting the endogenous X-linked MECP2 locus, we introduced four independent missense mutations that cause the autism spectrum disorder Rett syndrome and observed the desired genetic structure in 3-26% of selected clones, including gene targeting of the inactive X chromosome. Similar efficiencies were achieved by introducing neurodevelopmental disorder-causing mutations at the autosomal EEF1A2 locus on chromosome 20. Our results indicate that efficiency of genetic "knock-in" is determined by the location of the mutation within the donor DNA molecule. Furthermore, we successfully introduced an mCherry tag at the MECP2 locus to yield a fusion protein, demonstrating that larger insertions are also straightforward in this system. We suggest that our optimised methods for altering the genome of LUHMES cells make them an attractive model for the study of neurogenetic disorders.

Targeted Genome Editing via CRISPR in the Pathogen Cryptococcus neoformans.

Low rates of homologous integration have hindered molecular genetic studies in Cryptococcus neoformans over the past 20 years, and new tools that facilitate genome manipulation in this important pathogen are greatly needed. To this end, we have investigated the use of a Class 2 CRISPR system in C. neoformans (formerly C. neoformans var. grubii). We first expressed a derivative of the Streptococcus pyogenes Cas9 nuclease in C. neoformans, and showed that it has no effect on growth, production of virulence factors in vitro, or virulence in a murine inhalation model. In proof of principle experiments, we tested the CAS9 construct in combination with multiple self-cleaving guide RNAs targeting the well-characterized phosphoribosylaminoamidazole carboxylase-encoding ADE2 gene. Utilizing combinations of transient and stable expression of our constructs, we revealed that functionality of our CRISPR constructs in C. neoformans is dependent upon the CAS9 construct being stably integrated into the genome, whilst transient expression of the guide RNA is sufficient to enhance rates of homologous recombination in the CAS9 genetic background. Given that the presence of the CRISPR nuclease does not influence virulence in a murine inhalation model, we have successfully demonstrated that this system is compatible with studies of C. neoformans pathogenesis and represents a powerful tool that can be exploited by researchers in the field.

Construction of bromodomain-deleted BRD7 mutation vector based on homologous recombination and reverse PCR amplification

To construct a eukaryotic expression vector of bromodomain-containing protein 7 (BRD7) with deletion of bromodomain (BRD7△brd) using the homologous recombination and reverse PCR amplification techniques. The linear DNA fragments of bromodomain-deleted mutation of BRD7 (pIRES2-EGFP- 3Flag/BRD7△brd) were amplified by one pair of reverse PCR primers using high-fidelity enzyme, and then these fragments were transformed into E.coli to obtain the eukaryotic expression vector expressing BRD7△brd protein based on homologous recombination and plasmid cyclization. Bromodomain-deleted clones were identified by digestion with restrictive enzymes, and then the sequence and protein expression were further confirmed by sequencing and Western blot assays. The results suggest that pIRES2-EGFP-3Flag/BRD7△brd was successfully constructed. We establish a simple and quick method to construct plasmids with pIRES2-EGFP- 3Flag/BRD7△brd using reverse PCR amplification and homologous recombination techniques. We also found that the concentration of template in PCR reaction system is one of the critical factors that affect the rate of homologous recombination. Of all, this improved technique could be widely used in the construction of gene mutations.

Genetic Engineering of an Unconventional Yeast for Renewable Biofuel and Biochemical Production.

Yarrowia lipolytica is a non-pathogenic, dimorphic and strictly aerobic yeast species. Owing to its distinctive physiological features and metabolic characteristics, this unconventional yeast is not only a good model for the study of the fundamental nature of fungal differentiation but is also a promising microbial platform for biochemical production and various biotechnological applications, which require extensive genetic manipulations. However, genetic manipulations of Y. lipolytica have been limited due to the lack of an efficient and stable genetic transformation system as well as very high rates of non-homologous recombination that can be mainly attributed to the KU70 gene. Here, we report an easy and rapid protocol for the efficient genetic transformation and for gene deletion in Y. lipolytica Po1g. First, a protocol for the efficient transformation of exogenous DNA into Y. lipolytica Po1g was established. Second, to achieve the enhanced double-crossover homologous recombination rate for further deletion of target genes, the KU70 gene was deleted by transforming a disruption cassette carrying 1 kb homology arms. Third, to demonstrate the enhanced gene deletion efficiency after deletion of the KU70 gene, we individually deleted 11 target genes encoding alcohol dehydrogenase and alcohol oxidase using the same procedures on the KU70 knockout platform strain. It was observed that the rate of precise homologous recombination increased substantially from less than 0.5% for deletion of the KU70 gene in Po1g to 33%-71% for the single gene deletion of the 11 target genes in Po1g KU70Δ. A replicative plasmid carrying the hygromycin B resistance marker and the Cre/LoxP system was constructed, and the selection marker gene in the yeast knockout strains was eventually removed by expression of Cre recombinase to facilitate multiple rounds of targeted genetic manipulations. The resulting single-gene deletion mutants have potential applications in biofuel and biochemical production.

Genetic Engineering of an Unconventional Yeast for Renewable Biofuel and Biochemical Production

Yarrowia lipolytica is a non-pathogenic, dimorphic and strictly aerobic yeast species. Owing to its distinctive physiological features and metabolic characteristics, this unconventional yeast is not only a good model for the study of the fundamental nature of fungal differentiation but is also a promising microbial platform for biochemical production and various biotechnological applications, which require extensive genetic manipulations. However, genetic manipulations of Y. lipolytica have been limited due to the lack of an efficient and stable genetic transformation system as well as very high rates of non-homologous recombination that can be mainly attributed to the KU70 gene. Here, we report an easy and rapid protocol for the efficient genetic transformation and for gene deletion in Y. lipolytica Po1g. First, a protocol for the efficient transformation of exogenous DNA into Y. lipolytica Po1g was established. Second, to achieve the enhanced double-crossover homologous recombination rate for further deletion of target genes, the KU70 gene was deleted by transforming a disruption cassette carrying 1 kb homology arms. Third, to demonstrate the enhanced gene deletion efficiency after deletion of the KU70 gene, we individually deleted 11 target genes encoding alcohol dehydrogenase and alcohol oxidase using the same procedures on the KU70 knockout platform strain. It was observed that the rate of precise homologous recombination increased substantially from less than 0.5% for deletion of the KU70 gene in Po1g to 33%-71% for the single gene deletion of the 11 target genes in Po1g KU70Δ. A replicative plasmid carrying the hygromycin B resistance marker and the Cre/LoxP system was constructed, and the selection marker gene in the yeast knockout strains was eventually removed by expression of Cre recombinase to facilitate multiple rounds of targeted genetic manipulations. The resulting single-gene deletion mutants have potential applications in biofuel and biochemical production.