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An innovative CRISPR/Cas9 mouse model of human isolated microtia indicates the potential contribution of CNVs near HMX1 gene.
BACKGROUND: Microtia is a prevalent congenital malformation, the precise etiology and pathogenesis of which remain elusive. Mutations in the non-coding region of the HMX1 gene have been implicated in isolated cases of microtia, emerging as a significant focus of contemporary research. Several pathogenic copy number variations (CNVs) proximal to the HMX1 gene have been documented in wild animal populations, whereas only a single large segmental duplication in this region has been identified in humans. However, the absence of a gene-edited animal model has impeded the investigation of the unclear gene function associated with HMX1 mutations in human isolated microtia. In this study, we sought to precisely identify the pathogenic mutation by analyzing three pedigrees alongside population controls. Subsequently, our objective was to develop a CRISPR/Cas9 gene-edited mouse model to elucidate the functional implications of the identified mutation. METHODS: Genomic DNA was collected from 32 affected individuals across three pedigrees, as well as from 2000 control subjects. Comprehensive genomic analyses, including genome-wide linkage analysis, targeted capture, second-generation sequencing, and copy number analysis, were conducted to identify potential mutations associated with congenital auricle malformation. CRISPR/Cas9 gene-edited murine models were generated in response to the identified mutation. The auricular phenotypes of these gene-edited mice were systematically monitored. Small-animal Micro-CT scanning was employed to identify potential craniofacial or skeletal abnormalities. Furthermore, the expression of the HMX1 gene in the PA2 region of mouse embryos was quantified using RT-qPCR. RESULTS: A co-segregated 600 base pair duplication located on chromosome 4 (chr4:8701900-8702500, hg19) was identified in affected individuals across three pedigrees, but was absent in healthy controls. Two types of CRISPR/Cas9 gene-edited mice were subsequently generated. The knock-in (KI) mouse model was engineered by inserting one copy of the duplicated sequence directly adjacent to the mutated site, whereas the knockout (KO) mouse model was created by excising the mutation sequence. The phenotypes of different group of CRISPR/Cas9 gene-edited mice demonstrated distinct auricular deformities. Furthermore, an increase in the copy number of the mutated sequence was associated with elevated expression levels of HMX1 in the gene-edited mouse model. CONCLUSIONS: In this study, we further narrowed down and identified a 600 base pair copy number variation (CNV) located at chr4:8701900-8702500 (hg19), which is implicated in human bilateral, isolated microtia. Utilizing CRISPR/Cas9 technology, we developed novel mouse models harboring the identified mutation. These models serve as a robust platform for the comprehensive investigation of the underlying mechanisms of the disease.
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CRISPR DNA elements controlling site-specific spacer integration and proper repeat length by a Type II CRISPR-Cas system.
CRISPR-Cas systems provide heritable immunity against viruses by capturing short invader DNA sequences, termed spacers, and incorporating them into the CRISPR loci of the prokaryotic host genome. Here, we investigate DNA elements that control accurate spacer uptake in the type II-A CRISPR locus of Streptococcus thermophilus. We determined that purified Cas1 and Cas2 proteins catalyze spacer integration with high specificity for CRISPR repeat junctions. We show that 10 bp of the CRISPR leader sequence is critical for stimulating polarized integration preferentially at the repeat proximal to the leader. Spacer integration proceeds through a two-step transesterification reaction where the 3' hydroxyl groups of the spacer target both repeat borders on opposite strands. The leader-proximal end of the repeat is preferentially targeted for the first site of integration through recognition of sequences spanning the leader-repeat junction. Subsequently, second-site integration at the leader-distal end of the repeat is specified by multiple determinants including a length-defining mechanism relying on a repeat element proximal to the second site of integration. Our results highlight the intrinsic ability of type II Cas1/Cas2 proteins to coordinate directional and site-specific spacer integration into the CRISPR locus to ensure precise duplication of the repeat required for CRISPR immunity.
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Correction of diverse muscular dystrophy mutations in human engineered heart muscle by single-site genome editing.
Genome editing with CRISPR/Cas9 is a promising new approach for correcting or mitigating disease-causing mutations. Duchenne muscular dystrophy (DMD) is associated with lethal degeneration of cardiac and skeletal muscle caused by more than 3000 different mutations in the X-linked dystrophin gene (DMD). Most of these mutations are clustered in "hotspots." There is a fortuitous correspondence between the eukaryotic splice acceptor and splice donor sequences and the protospacer adjacent motif sequences that govern prokaryotic CRISPR/Cas9 target gene recognition and cleavage. Taking advantage of this correspondence, we screened for optimal guide RNAs capable of introducing insertion/deletion (indel) mutations by nonhomologous end joining that abolish conserved RNA splice sites in 12 exons that potentially allow skipping of the most common mutant or out-of-frame DMD exons within or nearby mutational hotspots. We refer to the correction of DMD mutations by exon skipping as myoediting. In proof-of-concept studies, we performed myoediting in representative induced pluripotent stem cells from multiple patients with large deletions, point mutations, or duplications within the DMD gene and efficiently restored dystrophin protein expression in derivative cardiomyocytes. In three-dimensional engineered heart muscle (EHM), myoediting of DMD mutations restored dystrophin expression and the corresponding mechanical force of contraction. Correcting only a subset of cardiomyocytes (30 to 50%) was sufficient to rescue the mutant EHM phenotype to near-normal control levels. We conclude that abolishing conserved RNA splicing acceptor/donor sites and directing the splicing machinery to skip mutant or out-of-frame exons through myoediting allow correction of the cardiac abnormalities associated with DMD by eliminating the underlying genetic basis of the disease.
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Targeted, efficient sequence insertion and replacement in rice.
CRISPR-Cas9 methods have been applied to generate random insertions and deletions, large deletions, targeted insertions or replacements of short sequences, and precise base changes in plants1-7. However, versatile methods for targeted insertion or replacement of long sequences and genes, which are needed for functional genomics studies and trait improvement in crops, are few and largely depend on the use of selection markers8-11. Building on methods developed in mammalian cells12, we used chemically modified donor DNA and CRISPR-Cas9 to insert sequences of up to 2,049 base pairs (bp), including enhancers and promoters, into the rice genome at an efficiency of 25%. We also report a method for gene replacement that relies on homology-directed repair, chemically modified donor DNA and the presence of tandem repeats at target sites, achieving replacement with up to 130-bp sequences at 6.1% efficiency.
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A Cleavage-Responsive Stem-Loop Hairpin for Assaying Guide RNA Activity.
The scope of the CRISPR-Cas9 technology now reaches far beyond genomic engineering. While significant efforts are driving the evolution of this revolutionary biomedical tool, the in vitro cleavage assay remains the standard method implemented to validate the guide RNA that directs endonuclease Cas9 to a desired genomic target. Here, we report the development of an alternative guide RNA validation system called GUIDER. GUIDER features a hairpin loop structure with a proximal guanosine-rich unit, a distal fluorophore unit, and a gRNA-targeting stem component. Cleavage of GUIDER by its complementary RNA-guided Cas9 endonuclease complex yields a fluorescent emission at 525 nm, signaling effective cleavage of the hairpin structure. GUIDER was validated using the model gene target mpcsk9, and it was able to identify the gRNA that could most efficiently cleave the target mpcsk9 gene. The modular design of GUIDER should allow it to have broad applicability in validating gRNAs, and its fluorescent signal output offers a rapid, simple, and quantitative measure of Cas9-mediated DNA cleavage.
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Direct measurement of engineered cancer mutations and their transcriptional phenotypes in single cells.
Genome sequencing studies have identified numerous cancer mutations across a wide spectrum of tumor types, but determining the phenotypic consequence of these mutations remains a challenge. Here, we developed a high-throughput, multiplexed single-cell technology called TISCC-seq to engineer predesignated mutations in cells using CRISPR base editors, directly delineate their genotype among individual cells and determine each mutation's transcriptional phenotype. Long-read sequencing of the target gene's transcript identifies the engineered mutations, and the transcriptome profile from the same set of cells is simultaneously analyzed by short-read sequencing. Through integration, we determine the mutations' genotype and expression phenotype at single-cell resolution. Using cell lines, we engineer and evaluate the impact of >100 TP53 mutations on gene expression. Based on the single-cell gene expression, we classify the mutations as having a functionally significant phenotype.
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Applications of the CRISPR/Cas system beyond gene editing.
Since the discovery of the clustered regularly interspaced short palindromic repeats (CRISPR)/CRISPR-associated system (Cas) as a tool for gene editing a plethora of locus-specific as well as genome-wide approaches have been developed that allow efficient and reproducible manipulation of genomic sequences. However, the seemingly unbound potential of CRISPR/Cas does not stop with its utilization as a site-directed nuclease. Mutations in its catalytic centers render Cas9 (dCas9) a universal recruitment platform that can be utilized to control transcription, visualize DNA sequences, investigate in situ proteome compositions and manipulate epigenetic modifications at user-defined genomic loci. In this review, we give a comprehensive introduction and overview of the development, improvement and application of recent dCas9-based approaches.
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Role of circadian gene Clock during differentiation of mouse pluripotent stem cells.
Biological rhythms controlled by the circadian clock are absent in embryonic stem cells (ESCs). However, they start to develop during the differentiation of pluripotent ESCs to downstream cells. Conversely, biological rhythms in adult somatic cells disappear when they are reprogrammed into induced pluripotent stem cells (iPSCs). These studies indicated that the development of biological rhythms in ESCs might be closely associated with the maintenance and differentiation of ESCs. The core circadian gene Clock is essential for regulation of biological rhythms. Its role in the development of biological rhythms of ESCs is totally unknown. Here, we used CRISPR/CAS9-mediated genetic editing techniques, to completely knock out the Clock expression in mouse ESCs. By AP, teratoma formation, quantitative real-time PCR and Immunofluorescent staining, we did not find any difference between Clock knockout mESCs and wild type mESCs in morphology and pluripotent capability under the pluripotent state. In brief, these data indicated Clock did not influence the maintaining of pluripotent state. However, they exhibited decreased proliferation and increased apoptosis. Furthermore, the biological rhythms failed to develop in Clock knockout mESCs after spontaneous differentiation, which indicated that there was no compensational factor in most peripheral tissues as described in mice models before (DeBruyne et al., 2007b). After spontaneous differentiation, loss of CLOCK protein due to Clock gene silencing induced spontaneous differentiation of mESCs, indicating an exit from the pluripotent state, or its differentiating ability. Our findings indicate that the core circadian gene Clock may be essential during normal mESCs differentiation by regulating mESCs proliferation, apoptosis and activity.
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Potent CRISPR-Cas9 inhibitors from Staphylococcus genomes.
Anti-CRISPRs (Acrs) are small proteins that inhibit the RNA-guided DNA targeting activity of CRISPR-Cas enzymes. Encoded by bacteriophage and phage-derived bacterial genes, Acrs prevent CRISPR-mediated inhibition of phage infection and can also block CRISPR-Cas-mediated genome editing in eukaryotic cells. To identify Acrs capable of inhibiting Staphylococcus aureus Cas9 (SauCas9), an alternative to the most commonly used genome editing protein Streptococcus pyogenes Cas9 (SpyCas9), we used both self-targeting CRISPR screening and guilt-by-association genomic search strategies. Here we describe three potent inhibitors of SauCas9 that we name AcrIIA13, AcrIIA14, and AcrIIA15. These inhibitors share a conserved N-terminal sequence that is dispensable for DNA cleavage inhibition and have divergent C termini that are required in each case for inhibition of SauCas9-catalyzed DNA cleavage. In human cells, we observe robust inhibition of SauCas9-induced genome editing by AcrIIA13 and moderate inhibition by AcrIIA14 and AcrIIA15. We also find that the conserved N-terminal domain of AcrIIA13-AcrIIA15 binds to an inverted repeat sequence in the promoter of these Acr genes, consistent with its predicted helix-turn-helix DNA binding structure. These data demonstrate an effective strategy for Acr discovery and establish AcrIIA13-AcrIIA15 as unique bifunctional inhibitors of SauCas9.
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Reshuffling yeast chromosomes with CRISPR/Cas9.
Genome engineering is a powerful approach to study how chromosomal architecture impacts phenotypes. However, quantifying the fitness impact of translocations independently from the confounding effect of base substitutions has so far remained challenging. We report a novel application of the CRISPR/Cas9 technology allowing to generate with high efficiency both uniquely targeted and multiple concomitant reciprocal translocations in the yeast genome. Targeted translocations are constructed by inducing two double-strand breaks on different chromosomes and forcing the trans-chromosomal repair through homologous recombination by chimerical donor DNAs. Multiple translocations are generated from the induction of several DSBs in LTR repeated sequences and promoting repair using endogenous uncut LTR copies as template. All engineered translocations are markerless and scarless. Targeted translocations are produced at base pair resolution and can be sequentially generated one after the other. Multiple translocations result in a large diversity of karyotypes and are associated in many instances with the formation of unanticipated segmental duplications. To test the phenotypic impact of translocations, we first recapitulated in a lab strain the SSU1/ECM34 translocation providing increased sulphite resistance to wine isolates. Surprisingly, the same translocation in a laboratory strain resulted in decreased sulphite resistance. However, adding the repeated sequences that are present in the SSU1 promoter of the resistant wine strain induced sulphite resistance in the lab strain, yet to a lower level than that of the wine isolate, implying that additional polymorphisms also contribute to the phenotype. These findings illustrate the advantage brought by our technique to untangle the phenotypic impacts of structural variations from confounding effects of base substitutions. Secondly, we showed that strains with multiple translocations, even those devoid of unanticipated segmental duplications, display large phenotypic diversity in a wide range of environmental conditions, showing that simply reconfiguring chromosome architecture is sufficient to provide fitness advantages in stressful growth conditions.
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