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Coupling CRISPR scanning with targeted chromatin accessibility profiling using a double-stranded DNA deaminase.
Genome editing enables sequence-function profiling of endogenous cis-regulatory elements, driving understanding of their mechanisms. However, these approaches lack direct, scalable readouts of chromatin accessibility across long single-molecule chromatin fibers. Here we leverage double-stranded DNA cytidine deaminases to profile chromatin accessibility at endogenous loci of interest through targeted PCR and long-read sequencing, a method we term targeted deaminase-accessible chromatin sequencing (TDAC-seq). With high sequence coverage at targeted loci, TDAC-seq can be integrated with CRISPR perturbations to link genetic edits and their effects on chromatin accessibility on the same single chromatin fiber at single-nucleotide resolution. We employed TDAC-seq to parse CRISPR edits that activate fetal hemoglobin in human CD34+ hematopoietic stem and progenitor cells (HSPCs) during erythroid differentiation as well as in pooled CRISPR and base-editing screens tiling an enhancer controlling the globin locus. We further scaled the method to interrogate 947 variants in a GFI1B-linked enhancer associated with myeloproliferative neoplasm risk in a single pooled CRISPR experiment in CD34+ HSPCs. Together, TDAC-seq enables high-resolution sequence-function mapping of single-molecule chromatin fibers by genome editing.
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Next-generation forward genetic screens: uniting high-throughput perturbations with single-cell analysis.
Programmable genome-engineering technologies, such as CRISPR (clustered regularly interspaced short palindromic repeats) nucleases and massively parallel CRISPR screens that capitalize on this programmability, have transformed biomedical science. These screens connect genes and noncoding genome elements to disease-relevant phenotypes, but until recently have been limited to individual phenotypes such as growth or fluorescent reporters of gene expression. By pairing massively parallel screens with high-dimensional profiling of single-cell types/states, we can now measure how individual genetic perturbations or combinations of perturbations impact the cellular transcriptome, proteome, and epigenome. We review technologies that pair CRISPR screens with single-cell multiomics and the unique opportunities afforded by extending pooled screens using deep multimodal phenotyping.
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CRISPR Gene Editing in Yeast: An Experimental Protocol for an Upper-Division Undergraduate Laboratory Course.
Clustered regularly interspaced short palindromic repeats (CRISPR) are a revolutionary tool based on a bacterial acquired immune response system. CRISPR has gained widespread use for gene editing in a variety of organisms and is an increasingly valuable tool for basic genetic research, with far-reaching implications for medicine, agriculture, and industry. This lab is based on the premise that upper division undergraduate students enrolled in a Life Sciences curriculum must become familiar with cutting edge advances in biotechnology that have significant impact on society. Toward this goal, we developed a new hands-on laboratory exercise incorporating the use of CRISPR-Cas9 and homology directed repair (HDR) to edit two well-characterized genes in the budding yeast, Saccharomyces cerevisiae. The two genes edited in this exercise, Adenine2 (ADE2) and Sterile12 (STE12) affect metabolic and developmental processes, respectively. Editing the premature stop codons in these genes results in clearly identifiable phenotypes that can be assessed by students in a standard laboratory course setting. Making use of this basic eukaryotic model organism facilitates a laboratory exercise that is inexpensive, simple to organize, set up, and present to students. This exercise enables undergraduate students to initiate and follow-up on all stages of the CRISPR gene editing process, from identification of guide RNAs, amplification of an appropriate HDR fragment, and analysis of mutant phenotypes. The organization of this protocol also allows for easy modification, providing additional options for editing any expressed genes within the yeast genome to produce new mutations, or recovery of existing mutants to wild type. © 2018 International Union of Biochemistry and Molecular Biology, 46(6):592-601, 2018.
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Screening of CRISPR/Cas base editors to target the AMD high-risk Y402H complement factor H variant.
PURPOSE: To evaluate the efficacy of using a CRISPR/Cas-mediated strategy to correct a common high-risk allele that is associated with age-related macular degeneration (AMD; rs1061170; NM_000186.3:c.1204T>C; NP_000177.2:p.His402Tyr) in the complement factor H (CFH) gene. METHODS: A human embryonic kidney cell line (HEK293A) was engineered to contain the pathogenic risk variant for AMD (HEK293A-CFH). Several different base editor constructs (BE3, SaBE3, SaKKH-BE3, VQR-BE3, and Target-AID) and their respective single-guide RNA (sgRNA) expression cassettes targeting either the pathogenic risk variant allele in the CFH locus or the LacZ gene, as a negative control, were evaluated head-to-head for the incidence of a cytosine-to-thymine nucleotide correction. The base editor construct that showed appreciable editing activity was selected for further assessment in which the base-edited region was subjected to next-generation deep sequencing to quantify on-target and off-target editing efficacy. RESULTS: The tandem use of the Target-AID base editor and its respective sgRNA demonstrated a base editing efficiency of facilitating a cytosine-to-thymine nucleotide correction in 21.5% of the total sequencing reads. Additionally, the incidence of insertions and deletions (indels) was detected in only 0.15% of the sequencing reads with virtually no off-target effects evident across the top 11 predicted off-target sites containing at least one cytosine in the activity window (n = 3, pooled amplicons). CONCLUSIONS: CRISPR-mediated base editing can be used to facilitate a permanent and stably inherited cytosine-to-thymine nucleotide correction of the rs1061170 SNP in the CFH gene with minimal off-target effects.
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Targeting head and neck cancer epigenetics with CRISPR-dCas9: An emerging therapeutic approach.
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CRISPR-Cas9 Gene Editing for Sickle Cell Disease and β-Thalassemia. Reply.
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Developmental history and application of CRISPR in human disease.
Genome-editing tools are programmable artificial nucleases, mainly including zinc-finger nucleases, transcription activator-like effector nucleases and clustered regularly interspaced short palindromic repeat (CRISPR). By recognizing and cleaving specific DNA sequences, genome-editing tools make it possible to generate site-specific DNA double-strand breaks (DSBs) in the genome. DSBs will then be repaired by either error-prone nonhomologous end joining or high-fidelity homologous recombination mechanisms. Through these two different mechanisms, endogenous genes can be knocked out or precisely repaired/modified. Rapid developments in genome-editing tools, especially CRISPR, have revolutionized human disease models generation, for example, various zebrafish, mouse, rat, pig, monkey and human cell lines have been constructed. Here, we review the developmental history of CRISPR and its application in studies of human diseases. In addition, we also briefly discussed the therapeutic application of CRISPR in the near future.
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Spotlight on CRISPR in Strongyloides Parasitic Nematodes.
Parasitic nematodes are biomedically and economically important, but many are genetically intractable which limits our understanding of their molecular and cellular biology. Gang et al. report CRISPR/Cas9 genome editing in parasites of the genus Strongyloides, generating both knock-outs and knock-ins, and demonstrated heritability of the modifications, a crucial advance in the field.
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CRISPR-Cas systems in oral microbiome: From immune defense to physiological regulation.
The clustered regularly interspaced short palindromic repeats with CRISPR-associated proteins (CRISPR-Cas) system, found in bacteria and archaea, provides sequence-based adaptive immunity against mobile genetic elements, including phages and plasmids. The oral cavity contains approximately 700 prokaryote species harboring known CRISPR-Cas systems, including type I, type II, type III, type V, and type VI, and unidentified CRISPR-Cas systems. There is increasing evidence to suggest that different CRISPR-Cas systems in the human oral microbiome can affect bacterial physiology through different mechanisms. Here, we review the canonical and novel functions of the CRISPR-Cas system, including defense against the invasion of foreign mobile elements, biofilm formation, acquisition of resistance genes, DNA repair, regulation of interspecific competition and intraspecific diversification, stress responses, and gene expression regulation. Overall, the mechanisms involved in CRISPR-Cas systems and their effects on bacterial physiology provide new insights into our understanding of the function and application of methods (including gene editing, modulation of CRISPR-Cas by anti-CRISPR, antimicrobials) on the oral microbiome.
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Guide RNA engineering for versatile Cas9 functionality.
The Clustered Regularly Interspaced Short Palindromic Repeats system allows a single guide RNA (sgRNA) to direct a protein with combined helicase and nuclease activity to the DNA. Streptococcus pyogenes Cas9 (SpCas9), a CRISPR-associated protein, has revolutionized our ability to probe and edit the human genome in vitro and in vivo Arguably, the true modularity of the Cas9 platform is conferred through the ease of sgRNA programmability as well as the degree of modifications the sgRNA can tolerate without compromising its association with SpCas9 and function. In this review, we focus on the properties and recent engineering advances of the sgRNA component in Cas9-mediated genome targeting.
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