Efficient genetic editing of human intestinal organoids using ribonucleoprotein-based CRISPR
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ABSTRACT:
PROVIDER: PRJNA1009059 | ENA |
REPOSITORIES: ENA
Dataset's files
| Action | DRS | |||
|---|---|---|---|---|
| SRR25757213_1.fastq.gz | Fastqsanger.gz | |||
| SRR25757213_2.fastq.gz | Fastqsanger.gz | |||
| SRR25757214_1.fastq.gz | Fastqsanger.gz | |||
| SRR25757214_2.fastq.gz | Fastqsanger.gz | |||
| SRR25757215_1.fastq.gz | Fastqsanger.gz |
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Project description:Organoids are currently one of the most widely used ex vivo models in epithelial biology. Combined with genetic editing strategies, organoids offer a promise of rapid and efficient investigation of gene function in many models of human disease. However, to date, the editing efficiency of organoids with the use of non-viral electroporation methods has been only up to 30%, with implications for the subsequent need for selection including turnaround time and exhaustion or adaptation of the organoid population. Here, we describe an efficient method of intestinal organoid editing using a Ribonucleoprotein CRISPR-based approach. Editing efficiencies of up to 98% in target genes were robustly achieved across different anatomical gut locations and developmental timepoints from multiple patient samples with no observed off-target editing. The method allowed us to study the effect of the loss of the tumour suppressor gene, PTEN, in normal human intestinal cells. Analysis of PTEN deficient organoids defined phenotypes that likely relate to its tumour suppressive function in vivo, such as a proliferative advantage and increased organoid budding. Transcriptional profiling revealed differential expression of genes in pathways commonly known to be associated with PTEN loss including mTORC1 activation.
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Project description:The CRISPR-Cas9 system enables efficient sequence-specific mutagenesis for creating germline mutants of model organisms. Key constraints in vivo remain the expression and delivery of active Cas9-guideRNA ribonucleoprotein complexes (RNPs) with minimal toxicity, variable mutagenesis efficiencies depending on targeting sequence, and high mutation mosaicism. Here, we established in vitro-assembled, fluorescent Cas9-sgRNA RNPs in stabilizing salt solution to achieve maximal mutagenesis efficiency in zebrafish embryos. Sequence analysis of targeted loci in individual embryos reveals highly efficient bi-allelic mutagenesis that reaches saturation at several tested gene loci. Such virtually complete mutagenesis reveals preliminary loss-of-function phenotypes for candidate genes in somatic mutant embryos for subsequent generation of stable germline mutants. We further show efficient targeting of functional non-coding elements in gene-regulatory regions using saturating mutagenesis towards uncovering functional control elements in transgenic reporters and endogenous genes. Our results suggest that in vitro assembled, fluorescent Cas9-sgRNA RNPs provide a rapid reverse-genetics tool for direct and scalable loss-of-function studies beyond zebrafish applications.
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Project description:We evaluate CRISPR-based prime editing for application in organoids. First we model mutations in TP53 in intestinal and hepatocyte oganoids and determine the efficiency and accuracy of mutation induction on multiple targets. Then, to evaluate potential clinical applicability of prime editing we repair mutations in the CFTR channel that cause cystic fibrosis in intestinal organoids. First we repair the CFTR-F508del mutation which is the most common mutation in cystic fibrosis. Then we compare adenine base editing to prime editing by repairing the CFTR-R785* mutation using both strategies.
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Project description:Genome editing through the delivery of CRISPR/Cas9-ribonucleoprotein (Cas9-RNP) reduces unwanted gene targeting and avoids integrational mutagenesis that can occur through gene delivery strategies. Direct and efficient delivery of Cas9-RNP into the cytosol followed by translocation to the nucleus remains a challenge. Here, we report a remarkably highly efficient (∼90%) direct cytoplasmic/nuclear delivery of Cas9 protein complexed with a guide RNA (sgRNA) through the coengineering of Cas9 protein and carrier nanoparticles. This construct provides effective (∼30%) gene editing efficiency and opens up opportunities in studying genome dynamics.
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Project description:The CRISPR/Cas9 system has been employed to efficiently edit the genomes of diverse model organisms. CRISPR-mediated mouse genome editing is typically accomplished by microinjection of Cas9 DNA/RNA and single guide RNA (sgRNA) into zygotes to generate modified animals in one step. However, microinjection is a technically demanding, labor-intensive, and costly procedure with poor embryo viability. Here, we describe a simple and economic electroporation-based strategy to deliver Cas9/sgRNA ribonucleoproteins into mouse zygotes with 100% efficiency for in vivo genome editing. Our methodology, designated as CRISPR RNP Electroporation of Zygotes (CRISPR-EZ), enables highly efficient and high-throughput genome editing in vivo, with a significant improvement in embryo viability compared with microinjection. Using CRISPR-EZ, we generated a variety of editing schemes in mouse embryos, including indel (insertion/deletion) mutations, point mutations, large deletions, and small insertions. In a proof-of-principle experiment, we used CRISPR-EZ to target the tyrosinase (Tyr) gene, achieving 88% bi-allelic editing and 42% homology-directed repair-mediated precise sequence modification in live mice. Taken together, CRISPR-EZ is simple, economic, high throughput, and highly efficient with the potential to replace microinjection for in vivo genome editing in mice and possibly in other mammals.
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Project description:Gene editing with CRISPR/Cas9 is a powerful tool to study the function of target genes. Although this technology has demonstrated wide efficiency in many species, including fertilized zebrafish and medaka fish embryos when microinjected, its application to achieve efficient gene editing in cultured fish cells have met some difficulty. Here, we report an efficient and reliable approach to edit genes in cultured medaka (Oryzias latipes) fish cells using pre-formed gRNA-Cas9 ribonucleoprotein (RNP) complex. Both medaka fish haploid and diploid cells were transfected with the RNP complex by electroporation. Efficient gene editing was demonstrated by polymerase chain reaction (PCR) amplification of the target gene from genomic DNA and heteroduplex mobility assay carried out with polyacrylamide gel electrophoresis (PAGE). The heteroduplex bands caused by RNP cleavage and non-homologous end joining could be readily detected by PAGE. DNA sequencing confirmed that these heteroduplex bands contains the mutated target gene sequence. The average gene editing efficiency in haploid cells reached 50%, enabling us to generate a clonal cell line with ntrk3b gene mutation for further study. This RNP transfection method also works efficiently in diploid medaka cells, with the highest mutation efficiency of 61.5%. The specificity of this synthetic RNP CRISPR/Cas9 approach was verified by candidate off-target gene sequencing. Our result indicated that transfection of pre-formed gRNA-Cas9 RNP into fish cells is efficient and reliable to edit target genes in cultured medaka fish cells. This method will be very useful for gene function studies using cultured fish cells.
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Project description:Ex vivo gene editing in T cells and hematopoietic stem/progenitor cells (HSPCs) holds promise for treating diseases. Gene editing encompasses delivery of a programmable editor RNA or ribonucleoprotein, often achieved ex vivo by electroporation and, when aiming to homology-driven correction, of a DNA template often provided by viral vectors together with a nuclease editor. Whereas HSPCs activate robust p53-dependent DNA damage response (DDR) upon nuclease-based editing, the responses triggered in T cells remain poorly characterized. Here, we performed comprehensive multi-omics analyses and found that electroporation is the main culprit of cytotoxicity in T cells, causing death and cell cycle delay, perturbing metabolism and inducing inflammatory response. Nuclease RNA delivery by lipid nanoparticles (LNPs) nearly abolished cell death and ameliorated cell growth, improving tolerance to the procedure and yielding higher number of edited cells compared to electroporation. Transient transcriptomic changes upon LNP treatment were mostly caused by cellular loading with exogenous cholesterol, whose potentially detrimental impact could be overcome by limiting exposure. Notably, LNP-based HSPC editing dampened p53 pathway induction and supported higher clonogenic activity and similar or higher reconstitution by long-term repopulating HSPCs compared to electroporation, reaching comparable editing efficiencies. Overall, LNPs may allow efficient and harmless ex vivo gene editing in hematopoietic cells for treatment of human diseases.
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