Name: a rapid and facile pipeline for generating genomic point mutants in c. elegans using crispr/cas9 ribonucleoproteins
Uploaded: 2018-04-30T15:00:00
Description: Watch this Scientific Journal Video about A Rapid and Facile Pipeline for Generating Genomic Point Mutants in C. elegans Using CRISPR/Cas9 Ribonucleoproteins at JoVE.com

There are no conflicts of interest related to this report.

All animal care and experimental procedures followed the guideline from the National Institutes of Health and the Institutional Animal Care and Use Committee (IACUC) at the University of Michigan. Use RNase-free solutions and pipette tips throughout the protocol. Clean the working area, pipettes, tubes, and centrifuge with RNase Decontamination solution following the manufacturer guidelines (see Materials Table).
1. sgRNA Target Selection
<ol>
	<li>Using a web browser, open ...

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The CRISPR-Cas9 system is a powerful and effective tool for precisely modifying the genome of model organisms. Here, we demonstrate that chimeric sgRNAs20 coupled with ssODN HDR templates enable the highly efficient generation of genomic point mutations in C. elegans. Importantly, we demonstrate that RNP delivery produces high editing efficiency when fluorescence is used as a co-selection marker, highlighting the ease and reliability of the technique.
The major...

Recent technological advances have radically transformed and accelerated the ability to precisely engineer genomes. In particular, the CRISPR-Cas9 system, which relies on the RNA-guided endonuclease Cas9 to induce a double strand break (DSB) near the target sequence of interest, has been extensively used to accurately engineer the genome of the majority of model organisms used in biomedical research1,2,3,4. Significantly, the use of CRISPR-Cas9 has unlocked genome editing even in difficult species like C. elegans5. Regardless of species, generating point mutations with the CRISPR-Cas9 based genome editing system relies on three core components: 1) Cas9 endonuclease, 2) a single guide RNA (sgRNA) that directs the Cas9 endonuclease to a target sequence, and 3) a user designed homology-directed repair (HDR) template containing the desired edit(s) of interest2.
There are several methods that can be used to introduce the targeting sgRNA and Cas9 nuclease into cells including plasmid, RNA, and viral-based delivery methods6. Recently, direct delivery of pre-complexed sgRNA-Cas9 Ribonucleoproteins (RNPs) has emerged as a powerful and efficient tool in CRISPR-Cas9-based genome editing7. The direct delivery of pre-complexed CRISPR-Cas9 RNPs has several distinct advantages, namely: 1) RNPs bypass the need for cellular transcription and translation, 2) RNPs are rapidly cleared, which may increase specificity by reducing available time for off-target cleavage, and 3) RNPs contain no foreign DNA/RNA elements which circumvents the introduction of non-native sequences into the host genome through random integration. Together, these attributes likely provide a short-lived burst of on-target CRISPR editing while minimizing off-target effects.
We describe a simple and efficient protocol for introducing site-specific genomic changes in C. elegans. This protocol includes targeting sgRNA and single stranded oligonucleotide (ssODN) HDR template design, sgRNA-Cas9 RNP complexing and delivery, and a genotyping strategy for the unequivocal identification of properly edited animals. Using this strategy, not only can the desired site-specific changes be recovered, but other non-specific indel mutations may also be recovered. Thus, our strategy permits the generation of an allelic series using a single strategy, where both mono-allelic, bi-allelic, and indel mutants can be generated in the F1 generation.

<table border="0" cellpadding="0" cellspacing="0" width="1144">
	<tbody>
		<tr height="40">
			<td height="40" style="height:40px;width:359px;">CRISPRevolution sgRNA&#160; EZ Kit</td>
			<td style="width:216px;">Synthego Inc.</td>
			<td style="width:344px;"></td>
			<td style="width:227px;">chimeric sgRNA</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Nuclease-free TE</td>
			<td>Synthego Inc.</td>
			<td>provided with the sgRNA kit EZ kit</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Nuclease-free water</td>
			<td>Synthego Inc.</td>
			<td>provided with the sgRNA kit EZ kit</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">4 nmole Ultramer DNA Oligo</td>
			<td>Integrated DNA Technologies</td>
			<td></td>
			<td>ssODN HDR template</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Alt-R S.p. HiFi Cas9 Nuclease 3NLS</td>
			<td>Integrated DNA Technologies</td>
			<td>1078728</td>
			<td>Cas9 protein</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">pCFJ90&#160;</td>
			<td>Addgene</td>
			<td>19327</td>
			<td>Pmyo-2::mCherry Marker Plasmid</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">KCl</td>
			<td>Sigma</td>
			<td>P5405</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">HEPES</td>
			<td>Sigma</td>
			<td>H4034</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">DNA Clean &#38; Concentrator</td>
			<td>Zymo Research</td>
			<td>D4004</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Zymoclean Gel DNA Recovery Kit</td>
			<td>Zymo Research</td>
			<td>D4002</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Q5 Hot Start High-Fidelity 2X Master Mix</td>
			<td>New England Biolabs</td>
			<td>M0494L</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Proteinase K</td>
			<td>Sigma</td>
			<td>P2308</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Glass Borosilicate Glass Micropipettes</td>
			<td>Sutter Instruments</td>
			<td>BF100-78-10</td>
			<td>OD: 1.0mm. ID: 0.78mm</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Trizma Hydrochloride</td>
			<td>Sigma</td>
			<td>T5941</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">MgCl2</td>
			<td>Sigma</td>
			<td>M2393</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">NP-40</td>
			<td>Sigma</td>
			<td>74385</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Tween-20</td>
			<td>Fisher Scientific</td>
			<td>BP337-100</td>
			<td></td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">RNaseZap Decontamination Solution</td>
			<td>Fisher Scientific</td>
			<td>AM9780</td>
			<td></td>
		</tr>
	</tbody>
</table>

a rapid and facile pipeline for generating genomic point mutants in c. elegans using crispr/cas9 ribonucleoproteins

The clustered regularly interspersed palindromic repeats (CRISPR)-CRISPR-associated protein 9 (Cas9) prokaryotic adaptive immune defense system has been co-opted as a powerful tool for precise eukaryotic genome engineering. Here, we present a rapid and simple method using chimeric single guide RNAs (sgRNA) and CRISPR-Cas9 Ribonucleoproteins (RNPs) for the efficient and precise generation of genomic point mutations in C. elegans. We describe a pipeline for sgRNA target selection, homology-directed repair (HDR) template design, CRISPR-Cas9-RNP complexing and delivery, and a genotyping strategy that enables the robust and rapid identification of correctly edited animals. Our approach not only permits the facile generation and identification of desired genomic point mutant animals, but also facilitates the detection of other complex indel alleles in approximately 4 - 5 days with high efficiency and a reduced screening workload.

Mutations in human superoxide dismutase 1 (SOD1) account for ~10 - 20% of familial amyotrophic lateral sclerosis, a devastating neurodegenerative disease that invariably leads to paralysis and death17. Human SOD-1 is an evolutionarily conserved protein sharing 55% identity and 70% similarity with the C. elegans SOD-1 protein (Figure 1B). To demonstrate the simplicity, feasibility, and efficiency of the CRISPR-Cas9 RNP...

Watch this Scientific Journal Video about A Rapid and Facile Pipeline for Generating Genomic Point Mutants in C. elegans Using CRISPR/Cas9 Ribonucleoproteins at JoVE.com

A Rapid and Facile Pipeline for Generating Genomic Point Mutants in C. elegans Using CRISPR/Cas9 Ribonucleoproteins

Here, we present a method to engineer the genome of C. elegans using CRISPR-Cas9 ribonucleoproteins and homology dependent repair templates.

A Rapid and Facile Pipeline for Generating Genomic Point Mutants in C. elegans Using CRISPR/Cas9 Ribonucleoproteins

The clustered regularly interspersed palindromic repeats (CRISPR)-CRISPR-associated protein 9 (Cas9) prokaryotic adaptive immune defense system has been ...

The overall goal of this procedure is to generate genomic point mutations in C.Elegans using single stranded oligonucleotide homology directed repair templates and CRISPR/Cas9 ribonucleoproteins. This method can help answer key questions in the neuroscience field such as determining the pathological consequences of genetic variance associated with neurodegenerative disease. The main advantage of this technique is that genomic point mutations can be generated rapidly allowing for the functional study of genetic variance within the context of endoginous regulatory control while avoiding the caveats of protein overexpression.To carry out sgRNA target selection, open up the webpage shown here. Input approximately 60 base pairs of sequence flanking the desired edit of interest. After selecting the C.Elegans genome and the protospacer adjacent motif according to the text protocol, click submit.On the results page, choose the top ranked target sequence closest to the edit of interest. Upon receipt, centrifuge the lyophilized sgRNA containing tube at room temperature and at least 12, 000 g for one minute. Add 60 microliters of nuclease free TE to the tube and use a p200 pipette to gently resuspend by pipetting up and down 15 to 20 times.The final concentration is 50 micromolar. Design an ssODN HDR template containing the mutation of interest, a unique in frame restriction endonuclease site, a silent mutation of one or both of the Gs within the NGG PAM sequence and 50 base pair five prime and three prime homology arms flanking the first and last mutation. Upon receipt, centrifuge the lyophilized ssODN containing tube as just demonstrated then use nuclease free DD H20 to gently resuspend ssODN to a final concentration of 100 micromolar.To prepare an injection mix, centrifuge the reagents shown here at maximum speed and four degrees celsius for two minutes. In the order listed, add the reagents to a nuclease free PCR tube. Then use a p20 pipette to gently and thoroughly mix the contents.Incubate the tube at room temperature for ten minutes. After injecting P0 animals according to the text protocol, allow them to recover at room temperature for one to two hours on an OP50 seeded 35 millimeter NGM plate. Subsequently using a platinum wire worm pick transfer single injected P0 animals to individual OP50 seeded 35 millimeter NGM plates.Two days post injection use a fluorescent microscope to identify P0 plates containing F1 progeny, expressing mCherry in the pharynx. Choose three P0 plates that contain the most mCherry positive F1 animals. From each of the three selected P0 plates use a worm pick to single eight to 12 mCherry positive F1 animals for a total of 24 to 36 mCherry positive F1s.Allow individual F1s to self fertilize and lay eggs at room temperature for one to two days. After one to two days of egg laying, use a worm pick to transfer the F1s into individual PCR strip tube caps containing seven microliters of worm lysis buffer. Centrifuge the PCR tubes at maximum speed and room temperature for one minute to bring the animals to the bottom of the tube.Then freeze the tubes at negative 80 degrees celsius for one hour. Next lyse frozen worms in a thermocycler using the following program. Then set up a PCR master mix as shown in this table.Add 21 microliters of PCR master mix into clean PCR tubes then add four microliters of the worm lysis tube and mix well by pipetting. Then run the PCR program following the manufacturer's guidelines. Purify the PCR reactions using a DNA clean and concentrate kit following the manufacturer's instructions.Then dilute the DNA by adding 10 microliters of water to the spin column. After setting up the restriction enzyme master mix add 10 microliters to each cleaned PCR reaction and incubate the tubes at 37 degrees celsius for one to two hours. Then separate the digested PCR products on a 1.5%agarose gel using 1x TAE buffer at 120 volts.Examine enzyme digested samples for the presence of bands that indicate potential edited animals. After identifying potential edited animals use the remaining three microliters of worm lysis and repeat the PCR. Then immediately load the completed reactions on a 1%agarose gel before separating and extracting the band using a gel extraction kit.Using the F1 primer carry out Sanger sequencing to identify correctly edited animals. Finally to obtain homozygous animals from verified heterozygous edited animals, single eight to 12 F2 animals and carry out genotyping and sequence verification according to the text protocol. To demonstrate the simplicity, feasibility, and efficiency of the CRISPR/Cas9 RNP based approach, the C.Elegans sod-1 gene was targeted to introduce the disease associated human G93a variant in the worm genome.This gel image shows the genotyping results for 24 mCherry positive F1 animals. 10 contained monoallylic or biallylic modification, 10 were wild type, three were potential indels, and one was a PCR failure. To demonstrate that the fluorescent mCherry marker enriches for genome modification, eight mCherry negative animals from each of the three P0 plates were picked.Only one animal was correctly modified whereas 23 were wild type. This figure shows the chromatogram from the full length gel extracted PCR product demonstrating that the precise nucleotide changes designed in the ssODN HDR template were faithfully incorporated into the genome of this homozygous F1 animal. Once mastered, this technique can be utilized to generate and identify genomic point mutations in C.Elegans in four to five days if it is performed properly.While attempting this procedure it's important to remember to use nucleus free reagents and techniques including RNase free water, filter pipette tips, and gloves. Following this procedure, cellular, molecular, and behavioral assays can be performed in order to investigate phenotypes that may associate with the mutation of interest. After watching this video you should have a good understanding of how to precisely generate genomic point mutations in C.Elegans using chimeric single guide RNase and CRISPR/Cas9 ribonuclearproteins.

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Research

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Genetics

Optogenetic Random Mutagenesis Using Histone-miniSOG in C. elegans

Forward genetic screening in model organisms is the workhorse to discover functionally important genes and pathways in many biological processes. In most mutagenesis-based screens, researchers have relied on the use of toxic chemicals, carcinogens, or irradiation, which requires designated equipment, safety setup, and/or disposal of hazardous materials. We have developed a simple approach to induce heritable mutations in C. elegans using germline-expressed histone-miniSOG, a light-inducible potent generator of reactive oxygen species. This mutagenesis method is free of toxic chemicals and requires minimal laboratory safety and waste management. The induced DNA modifications include single-nucleotide changes and small deletions, and complement those caused by classical chemical mutagenesis. This methodology can also be used to induce integration of extrachromosomal transgenes. Here, we provide the details of the LED setup and protocols for standard mutagenesis and transgene integration.

Optogenetic Random Mutagenesis Using Histone-miniSOG in C. elegans

Genetically-encoded histone-miniSOG induces genome-wide heritable mutations in a blue&#160;light-dependent manner. This mutagenesis method is simple, fast, free of toxic chemicals, and well-suited for forward genetic screening and transgene integration.

Forward genetic screening in model organisms is the workhorse to discover functionally important genes and pathways in many biological processes. In most ...

Using a Fluorescent PCR-capillary Gel Electrophoresis Technique to Genotype CRISPR/Cas9-mediated Knockout Mutants in a High-throughput Format

The development of programmable genome-editing tools has facilitated the use of reverse genetics to understand the roles specific genomic sequences play in the functioning of cells and whole organisms. This cause has been tremendously aided by the recent introduction of the CRISPR/Cas9 system-a versatile tool that allows researchers to manipulate the genome and transcriptome in order to, among other things, knock out, knock down, or knock in genes in a targeted manner. For the purpose of knocking out a gene, CRISPR/Cas9-mediated double-strand breaks recruit the non-homologous end-joining DNA repair pathway to introduce the frameshift-causing insertion or deletion of nucleotides at the break site. However, an individual guide RNA may cause undesirable off-target effects, and to rule these out, the use of multiple guide RNAs is necessary. This multiplicity of targets also means that a high-volume screening of clones is required, which in turn begs the use of an efficient high-throughput technique to genotype the knockout clones. Current genotyping techniques either suffer from inherent limitations or incur high cost, hence rendering them unsuitable for high-throughput purposes. Here, we detail the protocol for using fluorescent PCR, which uses genomic DNA from crude cell lysate as a template, and then resolving the PCR fragments via capillary gel electrophoresis. This technique is accurate enough to differentiate one base-pair difference between fragments and hence is adequate in indicating the presence or absence of a frameshift in the coding sequence of the targeted gene. This precise knowledge effectively precludes the need for a confirmatory sequencing step and allows users to save time and cost in the process. Moreover, this technique has proven to be versatile in genotyping various mammalian cells of various tissue origins targeted by guide RNAs against numerous genes, as shown here and elsewhere.

The genotyping technique described here, which couples fluorescent polymerase chain reaction (PCR) to capillary gel electrophoresis, allows for high-throughput genotyping of nuclease-mediated knockout clones. It circumvents limitations faced by other genotyping techniques and is more cost effective than sequencing methods.

The development of programmable genome-editing tools has facilitated the use of reverse genetics to understand the roles specific genomic sequences play ...

Selection-dependent and Independent Generation of CRISPR/Cas9-mediated Gene Knockouts in Mammalian Cells

The CRISPR/Cas9 genome engineering system has revolutionized biology by allowing for precise genome editing with little effort. Guided by a single guide RNA (sgRNA) that confers specificity, the Cas9 protein cleaves both DNA strands at the targeted locus. The DNA break can trigger either non-homologous end joining (NHEJ) or homology directed repair (HDR). NHEJ can introduce small deletions or insertions which lead to frame-shift mutations, while HDR allows for larger and more precise perturbations. Here, we present protocols for generating knockout cell lines by coupling established CRISPR/Cas9 methods with two options for downstream selection/screening. The NHEJ approach uses a single sgRNA cut site and selection-independent screening, where protein production is assessed by dot immunoblot in a high-throughput manner. The HDR approach uses two sgRNA cut sites that span the gene of interest. Together with a provided HDR template, this method can achieve deletion of tens of kb, aided by the inserted selectable resistance marker. The appropriate applications and advantages of each method are discussed.

Recent advances in the ability to genetically manipulate somatic cell lines hold great potential for basic and applied research. Here, we present two approaches for CRISPR/Cas9 generated knockout production and screening in mammalian cell lines, with and without the use of selectable markers.

The CRISPR/Cas9 genome engineering system has revolutionized biology by allowing for precise genome editing with little effort. Guided by a single guide ...

Primordial Germ Cell Transplantation for CRISPR/Cas9-based Leapfrogging in Xenopus

The creation of mutant lines by genome editing is accelerating genetic analysis in many organisms. CRISPR/Cas9 methods have been adapted for use in the African clawed frog, Xenopus, a longstanding model organism for biomedical research. Traditional breeding schemes for creating homozygous mutant lines with CRISPR/Cas9-targeted mutagenesis have several time-consuming and laborious steps. To facilitate the creation of mutant embryos, particularly to overcome the obstacles associated with knocking out genes that are essential for embryogenesis, a new method called leapfrogging was developed. This technique leverages the robustness of Xenopus embryos to &#34;cut and paste&#34; embryological methods. Leapfrogging utilizes the transfer of primordial germ cells (PGCs) from efficiently-mutagenized donor embryos into PGC-ablated wildtype siblings. This method allows for the efficient mutation of essential genes by creating chimeric animals with wildtype somatic cells that carry a mutant germline. When two F0 animals carrying &#34;leapfrog transplants&#34; (i.e., mutant germ cells) are intercrossed, they produce homozygous, or compound heterozygous, null F1 embryos, thus saving a full generation time to obtain phenotypic data. Leapfrogging also provides a new approach for analyzing maternal effect genes, which are refractory to F0 phenotypic analysis following CRISPR/Cas9 mutagenesis. This manuscript details the method of leapfrogging, with special emphasis on how to successfully perform PGC transplantation.

Primordial Germ Cell Transplantation for CRISPR/Cas9-based Leapfrogging in Xenopus

Genes essential for survival pose technical hurdles for creating mutant lines. Leapfrogging circumvents lethality by combining genome editing with primordial germ cell transplantation to create wild-type animals carrying germline mutations. Leapfrogging also permits the efficient generation of homozygous null mutants in the F1 generation. Here, the transplantation step is demonstrated.

The creation of mutant lines by genome editing is accelerating genetic analysis in many organisms. CRISPR/Cas9 methods have been adapted for use in the ...

A Standard Methodology to Examine On-site Mutagenicity As a Function of Point Mutation Repair Catalyzed by CRISPR/Cas9 and SsODN in Human Cells

Combinatorial gene editing using CRISPR/Cas9 and single-stranded oligonucleotides is an effective strategy for the correction of single-base point mutations, which often are responsible for a variety of human inherited disorders. Using a well-established cell-based model system, the point mutation of a single-copy mutant eGFP gene integrated into HCT116 cells has been repaired using this combinatorial approach. The analysis of corrected and uncorrected cells reveals both the precision of gene editing and the development of genetic lesions, when indels are created in uncorrected cells in the DNA sequence surrounding the target site. Here, the specific methodology used to analyze this combinatorial approach to the gene editing of a point mutation, coupled with a detailed experimental strategy to measuring indel formation at the target site, is outlined. This protocol outlines a foundational approach and workflow for investigations aimed at developing CRISPR/Cas9-based gene editing for human therapy. The conclusion of this work is that on-site mutagenesis takes place as a result of CRISPR/Cas9 activity during the process of point mutation repair. This work puts in place a standardized methodology to identify the degree of mutagenesis, which should be an important and critical aspect of any approach destined for clinical implementation.

This protocol outlines the workflow of a CRISPR/Cas9-based gene editing system for the repair of point mutations in mammalian cells. Here, we use a combinatorial approach to gene editing with a detailed follow-on experimental strategy for measuring indel formation at the target site&#8212;in essence, analyzing onsite mutagenesis.

Combinatorial gene editing using CRISPR/Cas9 and single-stranded oligonucleotides is an effective strategy for the correction of single-base point ...

CRISPR/Cas9-mediated Targeted Integration In Vivo Using a Homology-mediated End Joining-based Strategy

As a promising genome editing platform, the CRISPR/Cas9 system has great potential for efficient genetic manipulation, especially for targeted integration of transgenes. However, due to the low efficiency of homologous recombination (HR) and various indel mutations of non-homologous end joining (NHEJ)-based strategies in non-dividing cells, in vivo genome editing remains a great challenge. Here, we describe a homology-mediated end joining (HMEJ)-based CRISPR/Cas9 system for efficient in vivo precise targeted integration. In this system, the targeted genome and the donor vector containing homology arms (~800 bp) flanked by single guide RNA (sgRNA) target sequences are cleaved by CRISPR/Cas9. This HMEJ-based strategy achieves efficient transgene integration in mouse zygotes, as well as in hepatocytes in vivo. Moreover, a HMEJ-based strategy offers an efficient approach for correction of fumarylacetoacetate hydrolase (Fah) mutation in the hepatocytes and rescues Fah-deficiency induced liver failure mice. Taken together, focusing on targeted integration, this HMEJ-based strategy provides a promising tool for a variety of applications, including generation of genetically modified animal models and targeted gene therapies.

CRISPR/Cas9-mediated Targeted Integration In Vivo Using a Homology-mediated End Joining-based Strategy

The clustered regularly interspaced short palindromic repeats/CRISPR associated protein 9 (CRISPR/Cas9) system provides a promising tool for genetic engineering, and opens up the possibility of targeted integration of transgenes. We describe a homology-mediated end joining (HMEJ)-based strategy for efficient DNA targeted integration in vivo and targeted gene therapies using CRISPR/Cas9.

As a promising genome editing platform, the CRISPR/Cas9 system has great potential for efficient genetic manipulation, especially for targeted integration ...

Highly Efficient Gene Disruption of Murine and Human Hematopoietic Progenitor Cells by CRISPR/Cas9

Advances in the hematopoietic stem cell (HSCs) field have been aided by methods to genetically engineer primary progenitor cells as well as animal models. Complete gene ablation in HSCs required the generation of knockout mice from which HSCs could be isolated, and gene ablation in primary human HSCs was not possible. Viral transduction could be used for knock-down approaches, but these suffered from variable efficacy. In general, genetic manipulation of human and mouse hematopoietic cells was hampered by low efficiencies and extensive time and cost commitments. Recently, CRISPR/Cas9 has dramatically expanded the ability to engineer the DNA of mammalian cells. However, the application of CRISPR/Cas9 to hematopoietic cells has been challenging, mainly due to their low transfection efficiencies, the toxicity of plasmid-based approaches and the slow turnaround time of virus-based protocols.
A rapid method to perform CRISPR/Cas9-mediated gene editing in murine and human hematopoietic stem and progenitor cells with knockout efficiencies of up to 90% is provided in this article. This approach utilizes a ribonucleoprotein (RNP) delivery strategy with a streamlined three-day workflow. The use of Cas9-sgRNA RNP allows for a hit-and-run approach, introducing no exogenous DNA sequences in the genome of edited cells and reducing off-target effects. The RNP-based method is fast and straightforward: it does not require cloning of sgRNAs, virus preparation or specific sgRNA chemical modification. With this protocol, scientists should be able to successfully generate knockouts of a gene of interest in primary hematopoietic cells within a week, including downtimes for oligonucleotide synthesis. This approach will allow a much broader group of users to adapt this protocol for their needs.

A protocol for fast CRISPR/Cas9-mediated gene disruption in mouse and human primary hematopoietic cells is described in this article. Cas9-sgRNA ribonucleoproteins are introduced via electroporation with sgRNAs generated through in vitro transcription and commercial Cas9. High editing efficiencies are achieved with limited time and financial cost.

Advances in the hematopoietic stem cell (HSCs) field have been aided by methods to genetically engineer primary progenitor cells as well as animal models. ...

CRISPR/Cas9 Gene Editing to Make Conditional Mutants of Human Malaria Parasite P. falciparum

Malaria is a significant cause of morbidity and mortality worldwide. This disease, which primarily affects those living in tropical and subtropical regions, is caused by infection with Plasmodium parasites. The development of more effective drugs to combat malaria can be accelerated by improving our understanding of the biology of this complex parasite. Genetic manipulation of these parasites is key to understanding their biology; however, historically the genome of P. falciparum has been difficult to manipulate. Recently, CRISPR/Cas9 genome editing has been utilized in malaria parasites, allowing for easier protein tagging, generation of conditional protein knockdowns, and deletion of genes. CRISPR/Cas9 genome editing has proven to be a powerful tool for advancing the field of malaria research. Here, we describe a CRISPR/Cas9 method for generating glmS-based conditional knockdown mutants in P. falciparum. This method is highly adaptable to other types of genetic manipulations, including protein tagging and gene knockouts.

CRISPR/Cas9 Gene Editing to Make Conditional Mutants of Human Malaria Parasite P. falciparum

We describe a method for generating glmS-based conditional knockdown mutants in Plasmodium falciparum using CRISPR/Cas9 genome editing.

Malaria is a significant cause of morbidity and mortality worldwide. This disease, which primarily affects those living in tropical and subtropical ...

Endogenous Protein Tagging in Human Induced Pluripotent Stem Cells Using CRISPR/Cas9

A protocol is presented for generating human induced pluripotent stem cells (hiPSCs) that express endogenous proteins fused to in-frame&#160;N- or C-terminal fluorescent tags. The prokaryotic CRISPR/Cas9 system (clustered regularly interspaced short palindromic repeats/CRISPR-associated 9) may be used to introduce large exogenous sequences into genomic loci via homology directed repair (HDR). To achieve the desired knock-in, this protocol employs the ribonucleoprotein (RNP)-based approach where wild type Streptococcus pyogenes Cas9 protein, synthetic 2-part guide RNA (gRNA), and a donor template plasmid are delivered to the cells via electroporation. Putatively edited cells expressing the fluorescently tagged proteins are enriched by fluorescence activated cell sorting (FACS). Clonal lines are then generated and can be analyzed for precise editing outcomes. By introducing the fluorescent tag at the genomic locus of the gene of interest, the resulting subcellular localization and dynamics of the fusion protein can be studied under endogenous regulatory control, a key improvement over conventional overexpression systems. The use of hiPSCs as a model system for gene tagging provides the opportunity to study the tagged proteins in diploid, nontransformed cells. Since hiPSCs can be differentiated into multiple cell types, this approach provides the opportunity to create and study tagged proteins in a variety of isogenic cellular contexts.

Described here is a protocol for tagging endogenously expressed proteins with fluorescent tags in human induced pluripotent stem cells using CRISPR/Cas9. Putatively edited cells are enriched by fluorescence activated cell sorting and clonal cell lines are generated.

A protocol is presented for generating human induced pluripotent stem cells (hiPSCs) that express endogenous proteins fused to in-frame&#160;N- or ...

CRISPR/Cas9 Ribonucleoprotein-mediated Precise Gene Editing by Tube Electroporation

Gene editing nucleases, represented by CRISPR-associated protein 9 (Cas9), are becoming mainstream tools in biomedical research. Successful delivery of CRISPR/Cas9 elements into the target cells by transfection is a prerequisite for efficient gene editing. This protocol demonstrates that tube electroporation (TE) machine-mediated delivery of CRISPR/Cas9 ribonucleoprotein (RNP), along with single-stranded oligodeoxynucleotide (ssODN) donor templates to different types of mammalian cells, leads to robust precise gene editing events. First, TE was applied to deliver CRISPR/Cas9 RNP and ssODNs to induce disease-causing mutations in the interleukin 2 receptor subunit gamma (IL2RG) gene and sepiapterin reductase (SPR) gene in rabbit fibroblast cells. Precise mutation rates of 3.57%-20% were achieved as determined by bacterial TA cloning sequencing. The same strategy was then used in human iPSCs on several clinically relevant genes including epidermal growth factor receptor (EGFR), myosin binding protein C, cardiac (Mybpc3), and hemoglobin subunit beta (HBB). Consistently, highly precise mutation rates were achieved (11.65%-37.92%) as determined by deep sequencing (DeepSeq). The present work demonstrates that tube electroporation of CRISPR/Cas9 RNP represents an efficient transfection protocol for gene editing in mammalian cells.

Presented here is a protocol for efficient CRISPR/Cas9 ribonucleoprotein-mediated gene editing in mammalian cells using tube electroporation.

Gene editing nucleases, represented by CRISPR-associated protein 9 (Cas9), are becoming mainstream tools in biomedical research. Successful delivery of ...