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AAV Vectorization of DSB-mediated Gene Editing Technologies.
Recent work both at the bench and the bedside demonstrate zinc-finger nucleases (ZFNs), CRISPR/Cas9, and other programmable site-specific endonuclease technologies are being successfully utilized within and alongside AAV vectors to induce therapeutically relevant levels of directed gene editing within the human chromosome. Studies from past decades acknowledge that AAV vector genomes are enhanced substrates for homology-directed repair in the presence or absence of targeted DNA damage within the host genome. Additionally, AAV vectors are currently the most efficient format for in vivo gene delivery with no vector related complications in >100 clinical trials for diverse diseases. At the same time, advancements in the design of custom-engineered site-specific endonucleases and the utilization of elucidated endonuclease formats have resulted in efficient and facile genetic engineering for basic science and for clinical therapies. AAV vectors and gene editing technologies are an obvious marriage, using AAV for the delivery of repair substrate and/or a gene encoding a designer endonuclease; however, while efficient delivery and enhanced gene targeting by vector genomes are advantageous, other attributes of AAV vectors are less desirable for gene editing technologies. This review summarizes the various roles that AAV vectors play in gene editing technologies and provides insight into its trending applications for the treatment of genetic diseases.
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Nucleofection-Based CRISPR/Cas Delivery in Human T Cells for Immunotherapy Applications.
Electroporation-based delivery of CRISPR/Cas systems has emerged as a powerful and versatile approach for gene editing in primary human T cells, enabling efficient, transient, and nonviral modification while minimizing genomic integration risks. This chapter focuses on the principles and practical implementation of electroporation (nucleofection) for the delivery of Cas9 ribonucleoprotein (RNP) complexes into human T cells, highlighting critical parameters that influence editing efficiency, cell viability, and scalability for research and clinical applications. We provide a comprehensive protocol for multiplex gene editing in primary human T cells using Cas9 RNP electroporation, including optimization of cell activation status, buffer composition, electroporation settings, and post-electroporation recovery. Particular emphasis is placed on strategies to achieve high-efficiency disruption of target loci such as TRAC and B2M, enabling the generation of edited T cell products with defined functional properties. As a representative application, we describe how this delivery platform can be integrated with chimeric antigen receptor (CAR) engineering to produce edited CAR-T cells, including universal "off-the-shelf" designs with reduced risks of graft-versus-host disease and immune rejection. Downstream evaluation methods, including multiparameter flow cytometry for assessing editing efficiency and immunophenotype, are also outlined.
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In vivo therapeutic genome editing via CRISPR/Cas9 magnetoplexes for myocardial infarction.
CRISPR/Cas9-mediated gene-editing technology has gained attention as a new therapeutic method for intractable diseases. However, the use of CRISPR/Cas9 for cardiac conditions such as myocardial infarction remains challenging due to technical and biological barriers, particularly difficulties in delivering the system and targeting genes in the heart. In the present study, we demonstrated the in vivo efficacy of the CRISPR/Cas9 magnetoplexes system for therapeutic genome editing in myocardial infarction. First, we developed CRISPR/Cas9 magnetoplexes that magnetically guided CRISPR/Cas9 system to the heart for efficient in vivo therapeutic gene targeting during heart failures. We then demonstrated that the in vivo gene targeting of miR34a via these CRISPR/Cas9 magnetoplexes in a mouse model of myocardial infarction significantly improved cardiac repair and regeneration to facilitate improvements in cardiac function. These results indicated that CRISPR/Cas9 magnetoplexes represent an effective in vivo therapeutic gene-targeting platform in the myocardial infarction of heart, and that this strategy may be applicable for the treatment of a broad range of cardiac failures.
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CRISPR target prediction remains blunt tool for clinical applications.
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Building the Class 2 CRISPR-Cas Arsenal.
Adaptation of CRISPR-Cas9 for genome-editing applications has revolutionized biomedical research. New single-component effector CRISPR systems are emerging from the bioinformatics pipeline. How can we best harness their power? Three new studies will no doubt facilitate this transition by generating the C2c1 and C2c2 structure snapshots in different functional states.
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CRISPR/Cas12a ribonucleoprotein mediated editing of tryptophan 2,3-dioxygenase of Spodoptera frugiperda.
In insect genome editing CRISPR/Cas9 is predominantly employed, while the potential of several classes of Cas enzymes such as Cas12a largely remain untested. As opposed to Cas9 which requires a GC-rich protospacer adjacent motif (PAM), Cas12a requires a T-rich PAM and causes staggered cleavage in the target DNA, opening possibilities for multiplexing. In this regard, the utility of Cas12a has been shown in only a few insect species such as fruit flies and the silkworm, but not in non-model insects such as the fall armyworm, Spodoptera frugiperda, a globally important invasive pest that defies most of the current management methods. In this regard, a more recent genetic biocontrol method known as the precision-guided sterile insect technique (pgSIT) has shown successful implementation in Drosophila melanogaster, with certain thematic adaptations required for application in agricultural pests. However, before the development of a controllable gene drive for a non-model species, it is important to validate the activity of Cas12a in that species. In the current study we have, for the first time, demonstrated the potential of Cas12a by editing an eye color gene, tryptophan 2,3-dioxygenase (TO) of S. frugiperda by microinjecting ribonucleoprotein complex into pre-blastoderm (G0) eggs. Analysis of G0 mutants revealed that all five mutants (two male and three female) exhibited distinct edits consisting of both deletion and insertion events. All five edits were further validated through in silico modeling to understand the changes at the protein level and further corroborate with the range of eye-color phenotypes observed in the present study.
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CRISPR/nCas9-Edited CD34+ Cells Rescue Mucopolysaccharidosis IVA Fibroblasts Phenotype.
Mucopolysaccharidosis (MPS) IVA is a bone-affecting lysosomal storage disease (LSD) caused by impaired degradation of the glycosaminoglycans (GAGs) keratan sulfate (KS) and chondroitin 6-sulfate (C6S) due to deficient N-acetylgalactosamine-6-sulfatase (GALNS) enzyme activity. Previously, we successfully developed and validated a CRISPR/nCas9-based gene therapy (GT) to insert an expression cassette at the AAVS1 and ROSA26 loci in human MPS IVA fibroblasts and MPS IVA mice, respectively. In this study, we have extended our approach to evaluate the effectiveness of our CRISPR/nCas9-based GT in editing human CD34+ cells to mediate cross-correction of MPS IVA fibroblasts. CD34+ cells were electroporated with the CRISPR/nCas9 system, targeting the AAVS1 locus. The nCas9-mediated on-target donor template insertion, and the stemness of the CRISPR/nCas-edited CD34+ cells was evaluated. Additionally, MPS IVA fibroblasts were co-cultured with CRISPR/nCas-edited CD34+ cells to assess cross-correction. CRISPR/nCas9-based gene editing did not affect the stemness of CD34+ cells but did lead to supraphysiological levels of the GALNS enzyme. Upon co-culture, MPS IVA fibroblasts displayed a significant increase in the GALNS enzyme activity along with lysosomal mass reduction, pro-oxidant profile amelioration, mitochondrial mass recovery, and pro-apoptotic and pro-inflammatory profile improvement. These results show the potential of our CRISPR/nCas9-based GT to edit CD34+ cells to mediate cross-correction.
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Expanding Horizons of CRISPR/Cas Technology: Clinical Advancements, Therapeutic Applications, and Challenges in Gene Therapy.
CRISPR-Cas technology has transformed the field of gene editing, opening new possibilities for treatment of various genetic disorders. Recent years have seen a surge in clinical trials using CRISPR-Cas-based therapies. This review examines the current landscape of CRISPR-Cas implementation in clinical trials, with data from key registries, including the Australian New Zealand Clinical Trials Registry, the Chinese Clinical Trial Register, and ClinicalTrials.gov. Emphasis is placed on the mechanism of action of tested therapies, the delivery method, and the most recent findings of each clinical trial.
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DNA-Free Genome Editing via Ribonucleoprotein (RNP) Delivery of CRISPR/Cas in Lettuce.
CRISPR/Cas9 nuclease system is getting popular in precise genome editing of both eukaryotic and prokaryotic systems due to its accuracy, programmability, and relative ease of use. CRISPR/Cas systems can be delivered into live cells via plasmid DNA, RNA, and ribonucleoprotein (RNP). Of these, the RNP method is of special interest due to enzymatic action in shorter time and controllability over their activity. In addition, because RNP does not involve DNA, none of unwanted DNA footprints are left in the host genome. Previously, we demonstrated that plant protoplasts can be transfected with functional RNPs and the whole plants can be regenerated from an engineered protoplast. Relative to the published methods, the revised protocols described here should help increase the success rate of whole plant regeneration by reducing damages to the naked protoplast cells.
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Efficient generation of stable, heritable gene edits in wheat using CRISPR/Cas9.
BACKGROUND: The use of CRISPR/Cas9 systems could prove to be a valuable tool in crop research, providing the ability to fully knockout gene function in complex genomes or to precisely adjust gene function by knockout of individual alleles. RESULTS: We compare gene editing in hexaploid wheat (Triticum aestivum) with diploid barley (Hordeum vulgare), using a combination of single genome and tri-genome targeting. High efficiency gene editing, 11-17% for single genome targeted guides and 5% for tri-genome targeted guides, was achieved in wheat using stable Agrobacterium-mediated transformation. Gene editing in wheat was shown to be predominantly heterozygous, edits were inherited in a Mendelian fashion over multiple generations and no off-target effects were observed. Comparison of editing between the two species demonstrated that more stable, heritable edits were produced in wheat, whilst barley exhibited continued and somatic editing. CONCLUSION: Our work shows the potential to obtain stable edited transgene-free wheat lines in 36 weeks through only two generations and that targeted mutagenesis of individual homeologues within the wheat genome is achievable with a modest amount of effort, and without off-target mutations or the need for lengthy crossing strategies.
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