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Found: 26 182
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A Novel CRISPR-Cas9 Strategy to Target DYSTROPHIN Mutations Downstream of Exon 44 in Patient-Specific DMD iPSCs.
Mutations in the DMD gene cause fatal Duchenne Muscular Dystrophy (DMD). An attractive therapeutic approach is autologous cell transplantation utilizing myogenic progenitors derived from induced pluripotent stem cells (iPSCs). Given that a significant number of DMD mutations occur between exons 45 and 55, we developed a gene knock-in approach to correct any mutations downstream of exon 44. We applied this approach to two DMD patient-specific iPSC lines carrying mutations in exons 45 and 51 and confirmed mini-DYSTROPHIN (mini-DYS) protein expression in corrected myotubes by western blot and immunofluorescence staining. Transplantation of gene-edited DMD iPSC-derived myogenic progenitors into NSG/mdx4Cv mice produced donor-derived myofibers, as shown by the dual expression of human DYSTROPHIN and LAMIN A/C. These findings further provide proof-of-concept for the use of programmable nucleases for the development of autologous iPSC-based therapy for muscular dystrophies.
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Magnetically Driven High-Speed Rolling Nanoclusters for Enhanced CRISPR/Cas9 Genome Editing.
Despite the tremendous potential of the CRISPR/Cas9 gene-editing technology in precision therapeutics, intracellular delivery remains a major challenge. High cytoplasmic viscosity and lysosomal entrapment significantly impair the cytosolic transport and gene-editing efficiency. In this study, we demonstrate that both the size and magnetic responsiveness of Fe3O4 nanoclusters can be finely tuned by modulating ionic strength, enabling their rapid propulsion under external magnetic fields. Leveraging this property, we develop magnetic nanoparticle cluster nanorobots (MagCbots) of approximately 200 nm in size by electrostatically assembling Fe3O4 nanoclusters with CRISPR-Cas9 plasmids. Under magnetic actuation, MagCbots exhibit rapid rotation in highly viscous intracellular environments, achieving a linear velocity of ∼0.41 μm/s. MagCbots reduce intracellular viscosity by approximately 50% and enhance lysosomal escape efficiency by 3-fold compared to nonactuated counterparts. Their porous architecture not only offers high payload capacity but also protects plasmid DNA from enzymatic degradation. Notably, MagCbots enable efficient genome editing of both PD1 and PLK1 genes across various cell lines including hard-to-transfect Jurkat T cells. This magnetically driven nanorobot platform presents a promising strategy for active intracellular delivery and holds significant potential for advancing gene therapy and related biomedical applications.
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CRISPR-Cas9 directed genome engineering for enhancing salt stress tolerance in rice.
Crop productivity in rice is harshly limited due to high concentration of salt in the soil. To understand the intricacies of the mechanism it is important to unravel the key pathways operating inside the plant cell. Emerging state-of-the art technologies have provided the tools to discover the key components inside the plant cell for salt tolerance. Among the molecular entities, transcription factors and/or other important components of sensing and signaling cascades have been the attractive targets and the role of NHX and SOS1 transporters amply described. Not only marker assisted programs but also transgenic approaches by using reverse genetic strategies (knockout or knockdown) or overexpression have been extensively used to engineer rice crop. CRISPR/Cas is an attractive paradigm and provides the feasibility for manipulating several genes simultaneously. Here, in this review we highlight some of the molecular entities that could be potentially targeted for generating rice amenable to sustain growth under high salinity conditions by employing CRISPR/Cas. We also try to address key questions for rice salt stress tolerance other than what is already known.
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A systematic genome-wide mapping of oncogenic mutation selection during CRISPR-Cas9 genome editing.
Recent studies have reported that genome editing by CRISPR-Cas9 induces a DNA damage response mediated by p53 in primary cells hampering their growth. This could lead to a selection of cells with pre-existing p53 mutations. In this study, employing an integrated computational and experimental framework, we systematically investigated the possibility of selection of additional cancer driver mutations during CRISPR-Cas9 gene editing. We first confirm the previous findings of the selection for pre-existing p53 mutations by CRISPR-Cas9. We next demonstrate that similar to p53, wildtype KRAS may also hamper the growth of Cas9-edited cells, potentially conferring a selective advantage to pre-existing KRAS-mutant cells. These selective effects are widespread, extending across cell-types and methods of CRISPR-Cas9 delivery and the strength of selection depends on the sgRNA sequence and the gene being edited. The selection for pre-existing p53 or KRAS mutations may confound CRISPR-Cas9 screens in cancer cells and more importantly, calls for monitoring patients undergoing CRISPR-Cas9-based editing for clinical therapeutics for pre-existing p53 and KRAS mutations.
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Structure-activity relationships study on inhibition of CRISPR-Cas9 by glycosaminoglycans.
The CRISPR-Cas9 system is a revolutionary genome editing system known for its precision, simplicity and efficiency, playing a crucial role in gene-editing. It has enabled applications ranging from biomedicine to agriculture. However, the uncontrollable activity of Cas9 has raised significant safety concerns in clinical settings, limiting its broader application. Consequently, regulating CRISPR-Cas9 activity holds substantial promise for enhancing the safety and efficacy of gene-editing technologies. In this study, we demonstrated that sulfated glycosaminoglycans (GAGs) exhibit inhibitory effects of Cas9. Specifically, both chondroitin sulfate (CS) and heparin (HP) can inhibit CRISPR/Cas9 activity, with heparin showing a stronger inhibitory effect that correlates positively with its concentration. Molecular dynamics simulations indicate that sulfated heparin residues might inhibit Cas9 function by binding to essential DNA-binding sites, which are crucial for functional interactions, potentially impairing activity. Additionally, higher molecular weight GAGs exhibit enhanced inhibitory effects under the same sulphation. Notably, the sulfation site also influenced activity. C6-sulfation of chondroitin sulfate is more favorable for Cas9 inhibition, and N-sulfation of heparin enhances its inhibitory effect on Cas9 activity. These findings provide valuable insights into the development of carbohydrate-based inhibitors for CRISPR-Cas9, offering a foundation for further exploration in this field.
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In vivo promoter engineering in plants: Are we ready?
Engineering plant promoter sequence for optimal expression of a gene has been a long standing goal for plant scientists. In recent times, Sequence Specific Nucleases (SSNs) like CRISPR/Cas9 are enabling researchers to achieve this goal, in vivo in the genome. It is well known that SSNs have met with unprecedented success in rapid transgene free crop improvement largely by targeting the coding sequence. Here, we discuss the strategies being employed by plant scientists in targeting SSNs to non-coding promoter regions/Cis Regulatory Elements (CRE). We collectively refer all such endeavors as in vivo promoter engineering (IPE). We further classify the IPE efforts into CRE addition, CRE deletion/disruption, promoter swap/insertion and targeted promoter polymorphism. Till date, IPE has proven useful in altering plant architecture in tomato, developing resistance against Xanthomonas sp in rice and citrus, and engineering drought tolerance in maize. However it is quite challenging to achieve predictable changes in gene expression using IPE at this point. In future years, data generated from high throughput techniques to investigate non coding genome may immensely augment the efforts in this direction. As IPE does not involve addition of the transgene for modifying crop traits, it will be relatively more conducive to public acceptance in crop improvement programs.
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Single nucleotide replacement in the Atlantic salmon genome using CRISPR/Cas9 and asymmetrical oligonucleotide donors.
BACKGROUND: New breeding technologies (NBT) using CRISPR/Cas9-induced homology directed repair (HDR) has the potential to expedite genetic improvement in aquaculture. The long generation time in Atlantic salmon makes breeding an unattractive solution to obtain homozygous mutants and improving the rates of perfect HDR in founder (F0) fish is thus required. Genome editing can represent small DNA changes down to single nucleotide replacements (SNR). This enables edits such as premature stop codons or single amino acid changes and may be used to obtain fish with traits favorable to aquaculture, e.g. disease resistance. A method for SNR has not yet been demonstrated in salmon. RESULTS: Using CRISPR/Cas9 and asymmetrical ODNs, we were able to perform precise SNR and introduce a premature stop codon in dnd in F0 salmon. Deep sequencing demonstrated up to 59.2% efficiency in single embryos. In addition, using the same asymmetrical ODN design, we inserted a FLAG element into slc45a2 and dnd, showing high individual perfect HDR efficiencies (up to 36.7 and 32.7%, respectively). CONCLUSIONS: In this work, we demonstrate that precise SNR and knock-in (KI) can be performed in F0 salmon embryos using asymmetrical oligonucleotide (ODN) donors. We suggest that HDR-induced SNR can be applied as a powerful NBT, allowing efficient introgression of favorable alleles and bypassing challenges associated with traditional selective breeding.
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A single-plasmid-based, easily curable CRISPR/Cas9 system for rapid, iterative genome editing in Pseudomonas putida KT2440.
BACKGROUND: Pseudomonas putida KT2440, a non-pathogenic soil bacterium, is a key platform strain in synthetic biology and industrial applications due to its robustness and metabolic versatility. Various systems have been developed for genome editing in P. putida, including transposon modules, integrative plasmids, recombineering systems, and CRISPR/Cas systems. However, rapid iterative genome editing is limited by complex and lengthy processes. RESULTS: We discovered that the pBBR1MCS2 plasmid carrying the CRISPR/Cas9 module could be easily cured in P. putida KT2440 at 30 oC. We then developed an all-in-one CRISPR/Cas9 system for yqhD and ech-vdh-fcs deletions, respectively, and further optimized the editing efficiency by varying homology arm lengths and target sites. Sequential gene deletions of vdh and vanAB were carried out rapidly using single-round processing and easy plasmid curing. This system's user-friendliness was validated by 3 researchers from two labs for 9 deletions, 3 substitutions, and 2 insertions. Finally, iterative genome editing was used to engineer P. putida for valencene biosynthesis, achieving a 10-fold increase in yield. CONCLUSIONS: We developed and applied a rapid all-in-one plasmid CRISPR/Cas9 system for genome editing in P. putida. This system requires less than 1.5 days for one edit due to simplified plasmid construction, electroporation and curing processes, thus accelerating the cycle of genome editing. To our knowledge, this is the fastest iterative genome editing system for P. putida. Using this system, we rapidly engineered P. putida for valencene biosynthesis for the first time, showcasing the system's potential for expanding biotechnological applications.
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Expanding genome editing scopes with artificial intelligence.
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In 'proof of concept,' CRISPR-edited chickens shrug off flu.
Edits to one gene can't completely stop infections, however.
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