Here, we describe an expansion of the typical DNA size limitations associated with CRISPR knock-in technology, more specifically, the physical extent to which mouse genomic DNA can be replaced with donor (in this case, human) DNA at an orthologous locus by zygotic injection. Driving our efforts was the desire to create a whole animal model that would replace 17 kilobase pairs (kbp) of the mouse Bcl2l11 gene with the corresponding 25-kbp segment of human BCL2L11, including a conditionally removable segment (2.9-kbp) of intron 2, a cryptic human exon immediately 3′ of this, and a native human exon some 20 kbp downstream. Using two methods, we first carried out the replacement by employing a combination of bacterial artificial chromosome recombineering, classic embryonic stem cell (ESC) targeting, dual selection, and recombinase-driven cassette removal (ESC/Blastocyst Approach). Using a unique second method, we employed the same vector (devoid of its selectable marker cassettes), microinjecting it along with redundant single guide RNAs (sgRNAs) and Cas9 mRNA into mouse zygotes (CRISPR/Zygote Approach). In both instances, we were able to achieve humanization of Bcl2l11 to the extent designed, remove all selection cassettes, and demonstrate the functionality of the conditionally removable, loxP-flanked, 2.9-kbp intronic segment.
The discovery of clustered regularly interspaced short palindromic repeat (CRISPR) systems, the elucidation of their function, and their exploitation as genome engineering tools are revolutionizing genetic engineering1,2,3,4,5. Discovered as a form of adaptive immunity in bacteria and archaea, CRISPR systems consist of a series of DNA spacer elements derived from invading plasmids or viruses. Interdigitated among the spacers is a series of direct repeats. Depending on the particular system, these series are transcribed and processed into single spacer/repeat units called crRNAs (CRISPR RNAs). In turn, these crRNAs may interact with other short RNAs (e.g., tracrRNA) and one or more CRISPR-associated (Cas) proteins (e.g., CAS9 of Streptococcus pyogenes), culminating in the assembly of an RNA-guided endonuclease directed at degrading DNA from the offending plasmid or virus.
As genome engineering tools, the CRISPR-Cas endonucleases serve as instruments for generating DNA double-strand breaks (DSBs) with locus-of-interest specificity, at high frequency, and across a wide variety of strains and organisms6. When faced with DSBs, cells of the organism being perturbed may respond with a number of DNA repair pathways including the non-homologous end joining (NHEJ) pathway and the homology-directed repair (HDR) pathway7,8,9. DNA DSBs repaired by the efficient but error-prone NHEJ pathway are characterized by the deletion or insertion of a small number of nucleotides. As one might expect, these insertion/deletion events (INDELS), within the open reading frame of a protein of interest, may lead to the deletion of one or more endogenous amino acids, the insertion of one or more non-native amino acids, premature termination, or frameshift mutations. In each of these instances the modified mutant locus will commonly encode a hypomorphic or null allele of the original gene of interest.
In contrast, DSBs repaired in the presence of a homologous template (e.g., sister chromatid, donor molecule) may be repaired by homologous recombination (HR; a type of HDR)10. For genetic engineers, this provides the opportunity to introduce precise DNA modifications, created at the laboratory bench, into the organism under investigation, at the site of the DSB.
For classical gene-targeting, of the sort in use in the mouse for the past thirty years11,12,13,14,15, the typical paradigm, based on a large body of literature, has been to create plasmid vectors with two homology arms of a few to several kilobase pairs in length to act as donor molecules16,17. These arms are situated within the plasmid so as to flank investigator-altered sequences that will be incorporated into the genome after introduction of the plasmid vector into embryonic stem cells (ESCs) and homologous recombination. Positive and negative selection cassettes are frequently employed to aid in selecting the rare ESC clones containing properly integrated sequences. This technique is sufficient for modifying genomic sequence on a scale from one nucleotide to several thousand base pairs. The method may fall short, however, when attempting to alter entire mouse genes that often extend over 10 s or 100 s of thousands of base pairs.
In these instances, other genetic engineering technologies are employed including such methods as random transgenesis18,19, targeted transgenesis20,21, and recombinase-mediated cassette exchange (RMCE)22,23. Each of these methods has its drawbacks as well. For example, random transgenic methods deviate from genome modification at the cognate endogenous locus, sufficing to allow transgenes to integrate randomly (where they are subject to variegated expression). During targeted transgenesis, transgenes may be directed specifically to standardized safe harbor sites to limit this position-effect variegation but even here the transgenes are unlinked to their endogenous cognate genes. Like the related RMCE method, targeted transgenesis may involve the use of antibiotic selection cassettes flanked by recombinase-binding sites. In addition to the added complexity, deleting these selection cassettes requires breeding to specific recombinase-expressing mice thereby prolonging strain development24,25,26,27.
With the advent of CRISPR technologies many new avenues have opened28. For example, by dramatically increasing the frequency of DSBs at specified sites, gene-targeting need no longer be married to the culture of ESCs or the use and removal of selection cassettes29. In fact, in mice, most experiments begin with the microinjection of Cas9 mRNA and single guide RNAs (sgRNAs), (and when needed, donor molecules) into single-cell zygotes30. Furthermore, in species where ESC technology is lacking, CRISPR technology is a viable alternative, a fact that has opened gene-editing experimentation to a wide variety of strains and a broad range of species from bacteria to humans6. However, here again, DNA modifications have generally been limited to physical extents on the order of a few to a few thousand base pairs. Moreover, the effect of homology arm length on CRISPR-associated HR is only beginning to be elucidated31.
One interesting new approach is that of Yoshimi, et al.32, that sidesteps HR altogether. With this method donor molecules are injected into zygotes along with sgRNAs and single-stranded oligodeoxynucleotides (ssODNs). Donor molecules integrate seamlessly, presumably by a process of ssODN-mediated end joining.
In an effort to complement approaches such as those described above, we sought to test the limits of HR-mediated CRISPR knock-in technology, despite the associated technical uncertainties. Specifically, we aimed to test the physical extent to which mouse genomic DNA could be replaced with donor (in this case, human) DNA at an orthologous locus. Driving our efforts was the desire to create a whole animal model that would replace 17 kbp of the mouse Bcl2l11 gene with the corresponding segment of human BCL2L11, including a conditionally removable segment (2.9-kbp) of intron 2, a cryptic human exon immediately 3′ of this, and a native human exon some 20 kbp downstream (Fig. 1)33. Using two approaches, we first carried out the replacement by employing a combination of bacterial artificial chromosome (BAC) recombineering, classic ESC targeting, dual selection, and recombinase-driven cassette removal (Fig. 2a; hereafter referred to as our ESC/Blastocyst Approach)34. In the second approach, we used the same vector (devoid of its selectable marker cassettes), microinjecting it along with redundant sgRNA guides and Cas9 mRNA into mouse zygotes (Fig. 2b; hereafter referred to as our CRISPR/Zygote Approach). In both instances, we were able to achieve humanization of Bcl2l11 to the extent designed, remove all selection cassettes, and demonstrate the functionality of the conditionally removable, loxP-flanked, 2.9-kbp intronic segment.
Our latter result represents one of the largest segments of mouse DNA to be replaced by an orthologous human DNA using a CRISPR-directed approach with zygotic injection, to date. This study confirms that a minimum of at least 25 kbp of genomic DNA can be effectively humanized in mouse, and provides a foundation for further technical optimization in mouse and specialization for use in other species.
All mice were obtained from The Jackson Laboratory (JAX; Bar Harbor, ME, USA), housed on a bedding of white pine shavings, and fed NIH-31 5K52 (6% fat) diet and acidified water (pH 2.5 to 3.0), ad libitum. All experiments were performed with the approval of The Jackson Laboratory Institutional Animal Care and Use Committee (IACUC) and in compliance with the Guide for the Care and Use of Laboratory Animals (8th edition) and all applicable laws and regulations. The findings presented here have been prepared in close accordance with the ARRIVE Guidelines for reporting research performed in vivo35.
Preparation of the targeting vectors/donor molecules
We designed targeting vectors/donor molecules (Fig. 2a,b) with three objectives in mind — 1), to humanize a central segment of the BCL2L11/Bcl2l11 gene; 2), to place selectable markers immediately 5′ and 3′ of the humanized segment; and 3), to flank a 2,903-bp region within one of the humanized introns with loxP sites in order to model a disease-associated deletion observed in 12% of the East Asian population33.
Specifically, we constructed targeting vectors/donor molecules containing a 27,282-bp central segment of the human BCL2L11 gene flanked by 12,773- and 26,632-bp homology arms (consisting of the proximal and distal regions of the mouse Bcl2l11 gene), respectively. These constructs were designed such that they could be used both for homologous recombination in embryonic stem cells (ESCs), as well as for a CRISPR/Cas9 knock-in approach (Fig. 2a,b).
For our ESC/Blastocyst Approach, we electroporated 25 µg of linear pTLD39 DNA into 1.5 × 107 cells of the JM8-A3 (Strain: C57BL/6 N) line of mouse embryonic stems cells36. ESCs were plated, along with mitotically inactivated mouse embryonic fibroblasts (feeders), in ESC + 2i/LIF medium37 under selection with Geneticin® (G418, 200 µg/ml, Gibco, Fisher Thermo Scientific, Waltham, MA, USA) for seven days; or with puromycin (0.75 µg/ml, Sigma-Aldrich, St. Louis, MO, USA; three days on selection, four days off)37. Surviving ESC clones were propagated on ESC + 2i/LIF medium, karyotyped, further tested for the presence of the puromycin resistance cassette by PCR (oligonucleotides, Integrated DNA Technologies, Inc., Coralville, IA, USA; AccuStart II PCR SuperMix, Quantabio, Inc., Beverly, MA, USA; Eppendorf Mastercycler ep gradient, Eppendorf AG, Hamburg, DEU), and tentatively assessed for homology arm, human insert, and neomycin resistance cassette count by quantitative PCR. Properly targeted clones were microinjected into 3.5-days post coitum (dpc) blastocysts (see below).
For our CRISPR/Blastocyst Approach, all single-guide RNAs (sgRNAs) were designed using an algorithm available at http://crispr.mit.edu (August and October 2014; sequence type = unique genomic region; target genome = mouse, mm9)38. These sgRNAs, shown in Table 1, were designed along two concepts. In the first, the two highest scoring sgRNAs (with one in each orientation) within a 250-bp region were selected from both the 5′ and 3′ ends of the 17-kbp segment of the mouse Bcl2l11 segment being replaced. In the second, two internal sgRNAs (with one in each orientation) closest to each end of the replaced segment were selected regardless of their overall score. All sgRNAs were designed so as to not create DSBs within the donor vector. Additional detail on each of the sgRNAs is provided in the Supplementary Materials (Supplementary Fig. 2).
Guides were produced according to the method of Bassett, et al.39. Briefly, oligonucleotides encoding the T7 polymerase binding site and the sgRNA target sequence as well as an oligonucleotide encoding the remainder of the sgRNA sequence were ordered as 4 nmol Ultramers (Integrated DNA Technologies, Inc., Coralville, IA, USA). Guide templates were amplified with JumpStart Taq (Sigma-Aldrich, Corp., St. Louis, MO, USA), purified with a Qiagen PCR Purification Kit (Qiagen, Inc., Germantown, MD USA) and quantified by Nanodrop (ThermoFisher Scientific, Inc., Waltham, MA, USA). Transcription, purification and recovery were via MEGAshortscript and MEGAclear kits (Ambion/ThermoFisher Scientific, Inc., Waltham, MA, USA). Guides were analyzed for quality on the Bioanalyzer (Agilent Technologies, Inc., Santa Clara, CA, USA). Aliquots were frozen at −80′C until use. Cas9 mRNA (Streptococcus pyogenes SF370 mammalian codon-optimized CRISPR associated protein 9 mRNA, 5-methylcytidine, pseudouridine, Product Number L-6125) was purchased from TriLink Biotechnologies, Inc. (San Diego, CA, USA). Each set of sgRNAs (50 ng/µl), Cas9 mRNA (100 ng/µl), and donor DNA (10, 5, or 1 ng/µl) were assembled in a 25 µl volume with microinjection buffer (1 mM Tris-HCl, pH 7.5; 0.1 mM EDTA) (Table 2). The mixtures were centrifuged at 15,000 rpm for 15 minutes prior to microinjection.
For our ESC/Blastocyst Approach, properly targeted ESCs (12–15 cells per blastocyst) were microinjected into 3.5-dpc blastocysts (B6(Cg)-Tyrc−2J/J, JAX Stock # 000058) and the blastocysts transferred to pseudopregnant host dams (CByB6F1/J; JAX Stock # 100009), by standard techniques40. The resulting embryos were allowed to go to term; the pups were delivered naturally and reared by the dams until weaning at four weeks of age.
For our CRISPR/Zygote Approach, microinjection mixes were prepared as described above (Table 2). Approximately 80 C57BL/6NJ (JAX Stock # 005304) zygotes were microinjected (in one to two technical replicates with each microinjection mix described above), transferred to pseudopregnant females (CByB6F1/J) by standard techniques, and allowed to go to term where they were reared by the dams until weaning at four weeks of age.
C57BL/6J (JAX Stock # 000664) donor female mice (age 3 weeks) were superovulated to maximize embryo yield. Each donor female received five International Units (IU) of Pregnant Mare Serum Gonadotropin (PMSG, ProSpec HOR-272) intraperitoneally (IP), followed 47 hours later by 5 IU of human chorionic gonadotropin (hCG, ProSpec HOR-250), IP. Immediately post-administration of hCG, the female was mated with a single C57BL/6J stud male and was checked 22 hours later for the presence of a copulation plug. Females displaying a copulation plug were euthanized and the oviducts excised and placed into M2 medium. Prior to clutch collection the oviducts were placed in M2 medium containing hyaluronidase (Sigma H3506, 0.3 mg/mL). The oocyte clutch was removed by mechanically lysing the ampulla and the clutch was allowed to incubate in the hyaluronidase-containing M2 medium until the cumulus mass had disintegrated to the point of exposing the oocytes/prospective zygotes. The oocytes/prospective zygotes were then transferred through several washes of fresh M2 medium and then, through the process of visual grading, individual identified zygotes were separated and transferred to microdrops of K-RCVL (COOK K-RVCL) medium that were equilibrated under mineral oil (Sigma M8410) for 24 hours in a COOK MINC benchtop incubator (37°C, 5%CO2/5%O2/N2).
Zygotes were removed from culture and placed onto a slide containing 150 µL of fresh M2 medium. Microinjection was conducted on a Zeiss Axio Observer.D1 using Eppendorf NK2 micromanipulators in conjunction with Narashige IM-5A injectors. Standard zygote microinjection procedure was followed with special care made to deposit material (including circular vector) into the pronucleus of the subject zygote. Needles for microinjection were pulled fresh daily using WPI TW100F-4 capillary glass and a Sutter P97 horizontal puller. Injected zygotes were removed from the slide and rinsed through three 30 µL drops of equilibrated K-RCVL before being placed into a final 30 µL microdrop of equilibrated K-RCVL where they were subsequently processed for embryo transfer (via the oviduct) on the day of injection.
Zygotes processed for same day transfer were removed from culture and placed in a 1.8 mL screw-top tube (Thermo Scientific 363401) containing 900 µL of pre-warmed M2 medium for transport to the surgical station. The zygotes were removed from the tube and placed into culture (K-RCVL under oil, COOK MINC benchtop incubator 37 °C, 5%CO2/5%O2/N2). At the time of transfer the zygotes were removed from culture, placed into pre-warmed M2 medium, and transferred via the oviduct into 0.5 days post coitum (dpc) pseudopregnant CByB6F1/J females (age 9–11wks).
Potential founder (Generation P0) chimeric mice, arising from the microinjection of 3.5-dpc blastocysts (ESC/Blastocyst Approach) or 1-cell zygotes (CRISPR/Zygote Approach), and their progeny (Generation N1) were genotyped using the oligonucleotides described in Supplementary Table 2. As shown (Fig. 2a,b), these oligonucleotides were used in pairs, in separate PCR reactions designed to amplify DNA across: 1) the proximal (mPJ) and distal (mDJ) junctions, including CAS9 binding sites, of intact (or small INDEL-containing) mouse alleles, 2) the proximal (PJ) and distal (DJ) mouse/human junctions of humanized alleles (or randomly integrating transgenes), and 3) the breakpoints of any deletion-bearing (ΔJ) alleles. Proximal (P2.9), distal (D2.9), and deletion-spanning (Δ2.9) assays were designed around the 2.9-kbp polymorphism, as well. Other less likely forms of variation (larger deletions, inversions, etc.), although possible, were not assessed directly by genotyping.
For more detailed analysis of specific alleles, PCR products from genotyping reactions were purified and sequenced by JAX Scientific Services according to the method developed by Sanger41. PCR products were purified using HighPrep PCR magnetic beads (MagBio Genomics, Gaithersburg, MD USA). Cycle sequencing was performed using a BigDye Terminator Cycle Sequencing Kit, version 3.1 (Applied Biosystems, Foster City, CA USA). Sequencing reactions contained 5 µl of purified PCR product (3–20 ng) and 1 µl of oligonucleotide at a concentration of 5 pmol/µl. Sequencing reaction products were purified using HighPrep DTR (MagBio Genomics, Gaithersburg, MD USA). Purified reactions were run on an Applied Biosystems 3730xl DNA Analyzer (Applied Biosystems, Foster City, CA, USA). Sequence data were analyzed using Sequencing Analysis Software, version 5.2 (Applied Biosystems, Foster City, CA, USA). Resulting sequence (.abi) files were imported into Sequencher, version 5.0.1 (Gene Codes Corporation, Ann Arbor, MI, USA), for further analysis.
Droplet digital PCR
For mice of various genotypes derived from our most promising CRISPR founder, DNA samples were extracted from whole blood using the Qiagen QIAMP DNA mini kit (Qiagen, N.V., Venlo, NED), and quantified using a NanoDrop ND1000 spectrophotometer (ThermoFisher, Inc., Waltham, MA, USA). Copy number of the 5′ homology arm, 3′ homology arm, mouse Bcl2l11 gene, and human BCL2L11 gene was determined by Droplet Digital PCR (ddPCR) Copy Number Variation Assays (Bio-Rad Laboratories, Inc., Hercules, CA, USA). Each 22 µl PCR reaction contained 50 ng of DNA template, 10 µl of the ddPCR Supermix for probes (no dUTP), 1 µl of the FAM target oligonucleotides/probe (proprietary, Bio-Rad Laboratories), 1 µl of the HEX reference oligonucleotides/probe (proprietary, Bio-Rad Laboratories), and 10U HaeIII restriction enzyme (New England BioLabs, Ipswich, MA, USA). Droplets were generated on the QX200 Automated Droplet Generator, using the oil recommended for probes. Plates were heat-sealed with foil, using a PX1 PCR plate sealer set at 180 °C for 5 seconds. A C1000 Touch thermal cycler was used for PCR. Thermocycling conditions consisted of 1 cycle at 95 °C for 10 minutes, 40 cycles of denaturation at 94 °C for 30 seconds, with annealing and extension at 60 °C for 1 minute, and enzyme deactivation at 98 °C for 10 minutes. Droplets were read using a QX200 Droplet Reader. Analysis of the ddPCR data was performed using QuantaSoft software (version1.7.4.0917).
To show that the human segment of BCL2L11 had replaced its mouse counterpart in the orthologous Bcl2l11 locus, we used genetic mapping to localize the humanized segment of the BCL2L11/Bcl2l11 gene. Two backcrosses were established using the following approach. First, FVB/NJ (JAX Stock # 001800) females were crossed to C57BL/6NJ males carrying the humanized segment to obtain first-filial generation (F1) i.e., hybrid (FVB B6N F1/J) progeny. Progeny were then genotyped for the presence of the humanized segment. Males carrying the human sequence (FVB B6N F1/J-BCL2L11) were backcrossed to either FVB/NJ females or C57BL/6NJ females to generate second-generation backcross (N2) progeny.
These backcross schemes can be written as follows:
C57BL/6NJ X FVB B6N F1/J-BCL2L11
FVB/NJ X FVB B6N F1/J-BCL2L11
N2 progeny from each backcross (along with appropriate controls) were genotyped using KASP-chemistry (KASP chemistry is based on the use allele-specific primers with two distinct fluorophores that are quenched in the unamplified sample. After amplification, relief of quenching results in amplified fluorescence from the alleles present in each sample, be it allele 1, allele 2, or both. Details at http://www.lgcgroup.com; LGC Ltd., Teddington, UK) across a set of approximately 150 single-nucleotide polymorphism (SNP) markers (also available through LGC Ltd.) distributed roughly equally across the mouse genome (those from Chr 2 are further described in Supplementary Table 3). Concordance between each marker in the set and the humanized segment was calculated by chi-square (χ2) analysis.
Targeted locus amplification (TLA)
TLA was performed at Cergentis (Cergentis, B.V., Utrecht, Netherlands) according to the manufacturer’s recommendations. Each of three oligonucleotide sets (Fig. 2b) was used in individual TLA amplifications. PCR products were purified and libraries were prepared using the Illumina NexteraXT protocol (Illumina, Inc., San Diego, CA, USA) and sequenced on an Illumina sequencer.Reads were mapped to the mouse genome (mm 10) using BWA-SW, a Smith-Waterman alignment tool42. This allows partial mapping that is optimally suited for identifying break-spanning reads.
Data and materials availability
The mouse strains described in this work have been cryopreserved, or are maintained, at The Jackson Laboratory and may be accessed by contacting the corresponding author and mentioning JAX Stock (JR) # 27215, # 29083, and # 27561.
Final vector sequences described in this work have been deposited with GenBank and may be accessed under Accession Numbers MG711909 and MG711910. The vectors themselves have not been deposited with Addgene due to restrictions imposed by a Material Transfer Agreement with Children’s Hospital Oakland Research Institute (CHORI; Oakland, CA, USA), the source of mouse and human BACs used in vector construction.
Following electroporation of the pTLD39 vector into the JM8-A3 line of ESCs and selection on G418, we assayed 89 surviving clones for the presence of the puromycin resistance cassette by PCR. Of these, twenty-seven contained the puromycin cassette and were subjected to puromycin selection. Surprisingly, of these, only four clones survived to be assessed by quantitative PCR for homology arm, insert, and neomycin resistance cassette count (data not shown). One clone passed all of these tests for proper targeting of the central human BCL2L11 segment to the endogenous mouse Bcl2l11 gene. ESCs from this clone were microinjected into blastocysts resulting in nine high-quality (>50% chimerism as assessed by coat color) chimeras. The four highest quality male chimeras were mated to C57BL/6NJ females resulting in two independent instances of germline transmission of the humanized allele. Although presumably identical, independent lines (genetic background: C57BL/6JN) were developed from each instance. Mating males with B6N.Cg-Tg(Sox2-Cre)1Amc/J (JAX Stock # 014094) female mice resulted in progeny in which the loxP-flanked 2.9-kbp human intronic segment was deleted, as designed (Fig. 3).
In each of our CRISPR/Zygote Approach experiments, we employed four sgRNAs, two directed near the proximal end of the region of the mouse Bcl2l11 gene to be replaced and two directed near the distal end (Supplementary Fig. 2). In half of the experimental conditions that we tested, these four guides were those with the highest guide scores. In the remaining half of the experimental conditions that we tested, these four guides were those with the most terminal positions within the region of the mouse Bcl2l11 gene to be replaced (Table 2). We hypothesized that the redundancy of sgRNAs used in each of our experiments might be optimizing for (either or both of) the following reasons: first, that if one or the other sgRNA from a pair were inefficient at creating DSBs, the other might perform the task; and second, that if the creation and repair of DSBs were in a dynamic equilibrium, the presence of two closely spaced sgRNAs might cause DSBs to persist for a longer duration allowing more time for HR to occur. The results of these experiments are described here.
At term, a total of 89 pups were born of which five were stillborn and three did not survive to four weeks of age. The remaining eighty-one mice were weaned and are categorized among experiments as shown (Table 3).
Both Experiment 3 (highest scoring guides, 5 ng/µL donor DNA) and Experiment 5 (guides closest to ends, 10 ng/µL donor DNA) (Table 2) resulted in no viable pups remaining at wean-age (Supplementary Table 4). Despite these results Experiment 7 (conducted with a donor DNA concentration equal to that of Experiment 5, i.e., 10 ng/µL) and Experiment 8 (a replicate of Experiment 3) resulted in seven and 21 pups (at weaning), respectively, suggesting that the lack of pups in Experiments 3 and 5 was due to technical failure rather than anything systematically wrong with the experimental design.
To genotype these 81 progeny, PCR assays were designed to span each of the following regions: the proximal breakpoint of the mouse Bcl2l11 gene (PCR Assay mPJ), the distal breakpoint of the mouse Bcl2l11 gene (PCR Assay mDJ), the proximal mouse Bcl2l11/human BCL2L11 junction (PCR Assay PJ), the distal mouse Bcl2l11/human BCL2L11 junction (PCR Assay DJ), and the 17-kbp mouse region (to be replaced) were it deleted (PCR Assay ΔJ) (see Figs 2a,b, 3a–c, and Supplementary Table 2). The results of these experiments are shown (Table 4).
PCR assays mPJ and mDJ amplify the proximal and distal regions of the mouse Bcl2l11 gene, respectively, where the sgRNA pairs were designed to act. We sequenced these amplification products (Sanger method) to identify potential small insertion/deletion (INDEL) events. Although under all experimental conditions, apparently unmodified DNA was most commonly observed (range 81.1% to 100.0%), INDELs were observed for five of eight sgRNAs (2.3% to 18.9%). In many instances, sequenced products provided well-organized traces suggestive of mono-allelic amplification, the second allele presumably failing to amplify due to an underlying INDEL which had deleted an oligonucleotide binding site (Fig. 4, P0 animals # 4, 6, 9, and 17). In addition, in some instances, sequencing traces were consistent with the amplification of at least two alleles (Fig. 4, P0 animal # 19).
As further noted in Table 4, PCR assays designed to span each of the proximal (PJ) and distal (DJ) mouse/human junctions identified three founders that were positive for both (Experiment 2, guides closest to ends, 1 ng/µL donor DNA; Experiment 6, guides closest to ends, 5 ng/µL donor DNA; and Experiment 7, highest scoring guides, 10 ng/µL donor DNA). PCR assays designed to span the 17-kbp mouse region (ΔJ) to be replaced (were it deleted) identified two of the three founders described above (Experiment 6, guides closest to ends, 5 ng/µL donor DNA; and Experiment 7, highest scoring guides, 10 ng/µL donor DNA).
To further explore the inheritance of these genetic changes, we mated the founder mice (Generation P0) from Experiments 2 (PJ+ DJ+ ΔJ−), 6 (PJ+ DJ+ ΔJ+), and 7 (PJ+ DJ+ ΔJ+) to C57BL/6J mice and genotyped their progeny. The results of these analyses are shown in Table 5. As shown, the P0 mouse (male) from Experiment 2 (guides closest to ends, 1 ng/µL donor DNA), although PJ+ and DJ+, failed to transmit the humanized allele to any of 29 of its first-generation backcross (N1) progeny suggesting that the P0 mouse is mosaic with a germline consisting primarily of cells that do not harbor the humanization construct or anticipated deletion.
In contrast, the PJ+ DJ+ ΔJ+ P0 mouse (male) from Experiment 7 (highest scoring guides, 10 ng/µL donor DNA) transmitted its deletion-bearing allele (ΔJ+) to four of its 21 N1 progeny. This P0 mouse, however, did not transmit the human insertion-bearing allele (PJ+, DJ+) to any of these 21 mice again suggesting that the P0 mouse is mosaic with a germline consisting of relatively few human insertion-bearing cells.
Interestingly, the PJ+ DJ+ ΔJ+ P0 mouse (female) from Experiment 6 (guides closest to ends, 5 ng/µL donor DNA) transmitted either a human insertion-bearing allele PJ+ DJ+ ΔJ− or a deletion-bearing allele PJ− DJ− ΔJ+ to all of its 13 N1 progeny, but never both, implying that this animal is breeding as a true heterozygote with a genotype of both human insertion- and deletion-bearing alleles (PJ+ DJ+/ΔJ+) at the Bcl2l11 locus. Subsequent breeding of three select N1 mice, two bearing the human insertion (PJ+ DJ+ ΔJ−) and one bearing the deletion (PJ− DJ− ΔJ+), gave results consistent with Mendelian expectations. Mating males with B6N.Cg-Tg(Sox2-Cre)1Amc/J female mice resulted in progeny in which the loxP-flanked 2.9-kbp human intronic segment (Fig. 3d,e) was deleted (Fig. 3f), as designed.
Droplet digital PCR
To determine the copy number of various DNA segments associated with the integration and deletion events arising from the Experiment 6 founder, we raised mice with various preliminary genotypes and assessed the copy number of the 5′ homology arm, the 3′ homology arm, the mouse Bcl2l11 gene, and the human BCL2L11 gene by droplet digital PCR (ddPCR) (Fig. 5). For these experiments mouse genomic DNAs with the following preliminary genotypes were employed: a mouse Bcl2l11 deletion allele homozygote (Bcl2l11Δ/Bcl2l11Δ), a humanized BCL2L11 allele/mouse Bcl2l11 deletion allele heterozygote (BCL2L11h/Bcl2l11Δ), a humanized BCL2L11 allele homozygote (BCL2L11h/BCL2L11h, N = 2), a humanized BCL2L11 allele/wildtype mouse Bcl2l11 allele heterozygote (BCL2L11h/Bcl2l11m, N = 2), and a mouse wildtype Bcl2l11 allele homozygote (Bcl2l11m/Bcl2l11m).
In all instances, copy number of the 5′ homology arm, 3′ homology arm, mouse Bcl2l11 gene, and human BCL2L11 gene was as expected based on each animal’s preliminary genotype (Table 6).
We used an outcross-backcross genetic mapping strategy as a means of localizing the insertion site of BAC-derived human BCL2L11 sequences. Twenty-two N2 progeny were analyzed from the C57BL/6NJ X (FVB/NJ X C57BL/6NJ) backcross and twenty-eight progeny from the FVB/NJ X (FVB/NJ X C57BL/6NJ) backcross. Analysis of the data demonstrates strong linkage between the human BCL2L11 segment and several genetic markers on mouse Chromosome 2 (Fig. 6 and Supplementary Table 3). In the backcross to C57BL/6NJ, the marker with strongest linkage, marker rs13476756, had a log-odds ratio (LOD) of 6.58 (p < 0.004). In the backcross to FVB/NJ, marker rs13476756 had a LOD score of 7.64 (p < 0.0004).
Analysis of individual haplotypes (specifically, points of recombination in samples 261, 263, 266, 303, and 319) further narrows the insertion-critical region to a 45.2-Mbp region from marker rs4223406 (nucleotide 113,827,352) to marker rs3689600 (nucleotide 159,014,253) on Mouse Chromosome 2 (GRC38/mm10), which is consistent with integration into the 36,510-bp mouse Bcl2l11 gene that spans from nucleotide 128,126,038 to nucleotide 128,162,547. Put another way, this analysis shows that both the mouse Bcl2l11 gene and the engineered human sequences must be colocalized within a region comprising less than 2% of the mouse genome. We conclude that integration of the human sequence has not occurred randomly, but has indeed occurred by homologous recombination as designed.
Targeted locus amplification
Due to the large size of the homology arms (>15-kbp) used in our experiment, typical approaches used to confirm proper targeting (Southern blot analysis and long-range PCR) were untenable. Thus, to further address the issue of proper genomic targeting and the precise nature of the integration site, we turned to a more modern technique, targeted locus amplification (TLA)43.
TLA is a DNA crosslinking-based technique used to amplify tens of thousands of base-pairs in, and immediately surrounding, a locus of interest. When coupled with next-generation sequencing methods an entire locus of interest can be assessed at base-pair resolution.
We performed TLA with three amplicons (Fig. 2b and Supplementary Table 5) in the Bcl2l11/BCL2L11 targeted region — the first, at the 5′ end of the human BCL2L11 segment; the second, at the 3′ end of the human BCL2L11 segment; and third, in the 3′ (mouse) homology arm.
Recovered DNAs were sequenced and mapped to the mouse genome (mm10). As shown (Fig. 7a) the highest coverage of TLA reads, recovered using the 3′ human amplicon, is observed between 125 and 130 Mbp on Chr 2, indicating that the BCL2L11 containing targeting construct had integrated, as expected (i.e., within the general region of the mouse Bcl2l11 gene), and that there had been no off-target integration events in this line of mice. Similar results were obtained with the other two amplicons (data not shown).
More specifically, when coverage around the Bcl2l11 locus is analyzed at higher resolution, it can be seen that for each of the three amplicons individual TLA-recovered sequences localize to regions of the 5′ and 3′ mouse homology arms (Fig. 7b1) and, most important, some extend in a seamless fashion more laterally into areas of the genome immediately flanking the mouse homology arms, as expected (Fig. 7b2), but nowhere else.
No recovered sequences localize to the central region of the mouse Bcl2l11 gene, suggesting that the central region has been deleted (i.e., replaced) by the orthologous integrating human sequence. In fact, at the 5′ and 3′ extremes of the central region of Bcl2l11 to be replaced, local sequencing reads are chimeric, containing sequences from both the mouse Bcl2l11 and human BCL2L11 genes adjoining as originally designed in our targeting vector (Fig. 7c).
Moreover, when aligned to the sequence of our targeting vector itself, TLA-recovered sequences from each of the three amplicons localize across the construct, aligning with the 5′ mouse homology arm, the central region of the human BCL2L11 gene, and the 3′ homology arm, as designed (Fig. 7d1, d2).
Other evidence supporting presence of the designed integration event includes the absence of TLA-recovered sequence reads corresponding to the vector backbone, the absence of sequence reads indicating unexpected transgene/transgene fusions, and the absence of sequence reads indicating unexpected transgene/genome fusions.
Taking the data collectively, we conclude that the targeting construct introduced into zygotes (along with Cas9 mRNA and appropriate sgRNAs) has integrated seamlessly at the Bcl2l11 locus, humanizing the central portion of the gene, as designed.
Contemporary CRISPR technology is revolutionizing genetic engineering and has contributed [along with zinc-finger nuclease (ZFN) and transcription activator-like effector nuclease (TALEN) technologies] to the newly emergent field of gene editing38,44,45,46,47,48,49,50,51,52,53,54,55,56. The greater CRISPR technique is in a period of rapid expansion, its methodology now being applied across dozens of species57 in thousands of laboratories around the globe58. Moreover, the seminal core technology continues to diversify with additional enzymatic reagents, novel applications, and technical improvements under robust investigation. This, in turn, has led to a rapid expansion of CRISPR knowledge and the publication of CRISPR reports and reviews on a daily basis.
In the experiments reported here, we set out to explore the utility of using CRISPR technology in mouse zygotes, later brought to term, to replace large (10 s of kbp) segments of the mouse genome with human DNA from orthologous loci. Current CRISPR approaches aimed at knocking experimental DNAs into a locus of interest by homologous recombination have generally involved relatively small genomic expanses from single nucleotides to a few kilobase pairs. Moreover, these experiments routinely make use of long oligonucleotides, or targeting vectors with sub-kilobase homology arms, as donor molecules59. Only more rarely are targeting vectors used of the sizes routinely employed in studies involving mouse ESCs32.
In contrast to these common practices, we surmised that experimentally altered DNAs, of 10 s to 100 s of kilobase pair lengths, might be directed into a locus of interest if the DNA were outfitted with homology arms 15–30 times longer than those in common use today. Accordingly, we used both ESC and CRISPR Approaches with donor molecules containing 25-kbp of human BCL2L11 genomic sequence flanked by 15-kbp and 30-kbp mouse homology arms. In addition to success with the ESC/Blastocyst Approach, we have also demonstrated here (by PCR, sequence, and linkage analysis) that replacement of mouse genomic DNA can be achieved using human DNA (of at least 25-kbp) from the corresponding locus and a large vector/CRISPR-stimulated knock-in approach (CRISPR/Zygote Approach).
Given these results, future studies can now begin to explore questions of efficiency and optimization. In our experiment, we performed microinjection into mouse zygotes to see if mice could be recovered, with any degree of humanization of the mouse Bcl2l11 gene, and if these mice were capable of transmitting the humanized allele through the germline to their offspring. These experiments have demonstrated the utility of this CRISPR/BAC technology to introduce experimental DNA in a directed fashion to the zygotic genome and the ability of the specifically targeted DNA to be transmitted through the germline to progeny. However, due to the small number of data points in whole animal experiments, one can only speculate on the impact of guide selection and donor DNA concentration variables on overall success rates.
Among the experiments in which donor DNA was detected in P0 mice (Tables 3 and 4; Experiments 2, 6, and 7), DNA donor concentrations of 1, 5, and 10 ng/µL were represented but the resulting mice show varying degrees of mosaicism. In Experiment 2, where donor DNA concentration was at its lowest (1 ng/µL), donor DNA was not detected among N1 progeny (0/50) (Table 5) suggesting that integration of the donor DNA occurred at a multicellular stage of embryonic development and that those cells that did acquire the donor DNA did not contribute to the germline at an appreciable level.
In Experiment 6, where donor DNA concentration was at an intermediate level (5 ng/µL), donor DNA was detected among nearly half of all N1 progeny (14/31) suggesting that integration of the donor DNA occurred at the one-cell (zygotic) stage of embryonic development, that that cell gave rise to all cells of the germline, and that the donor DNA was passed, during meiosis, into half of the population of mature germ cells. This result is consistent with our hypothesis that a deletion (ΔJ+), of the 17-kbp mouse segment to be replaced, occurred at the Bcl2l11 locus in the homologous chromosome in the zygote, and was transmitted, in trans to the DNA insertion (PJ+, DJ+), to all remaining progeny (17/17). This result is entirely congruent with the optimal desired outcome, i.e., where the P0 zygote undergoes biallelic modification, develops into a mouse with no mosaicism, and transmits one or the other variant alleles in equal numbers (50%:50%) to the population of mature germ cells.
In Experiment 7, where donor DNA concentration was at the highest level tested (10 ng/µL), the 17-kbp deletion (ΔJ+) was detected in only 25% of all N1 progeny (14/56), and the donor DNA (PJ+, DJ+), present in the P0 mouse, was not transmitted to the N1 generation at all (0/56). These results can be explained assuming a scenario whereby a deletion occurred in one Bcl2l11 allele, in a single blastomere, at or near the two-cell stage, and that this deletion-bearing (ΔJ+) cell gave rise to roughly half of the developing premeiotic germline and a fourth of all mature (postmeiotic) germ cells. At some later point in blastogenesis, one can hypothesize that an insertion of donor DNA (PJ+, DJ+) occurred, but in so few cells as to not contribute to the germline in an appreciable way.
A number of aspects in Experiment 7 may have contributed to its less than optimal result. First, due to its viscosity, a donor DNA preparation with a DNA concentration that is too high may not be efficiently delivered through the microinjection needle to the zygote, or delivered in a form less conducive to promoting CAS9 activity and/or HR. Moreover, the guides designed for this experiment, although designed to have an optimal score, did not have what we surmised to be an optimal position, near the ends of the mouse DNA segment to be replaced. It may be that, in experiments of this type, guide position represents a more significant design parameter than guide activity alone.
It is interesting to note that, among all experiments using guides designed for high score optimization, only in Experiment 7, where donor DNA concentration was at the highest level tested (10 ng/µL), was any evidence of donor DNA incorporation (PJ+, DJ+) seen, and even here it was at a level apparently so low in the P0 founder mouse as to not transmit the modified allele to N1 mice. You may recall that, in the previously mentioned Experiment 6, where an optimal result was achieved, donor DNA concentration was only 5 ng/µL. It is entirely possible that the successful result seen in that instance was driven by superiorly performing/positioned (nearest the end) guides even at what could prove to be a suboptimal donor DNA concentration. Comparing Experiment 6 with Experiment 7, it is interesting to note that the experiment with the higher donor DNA concentration (Experiment 7, 10 ng/µL) did achieve a higher rate of incorporation (as a percentage of live born mice, 14.3% versus 5.6%) but a lower quality of allele modification in the single founder recovered (mosaicism/transmission of only one modified allele at low frequency compared to nonmosaicism/transmission of both modified alleles at maximum frequency). One may speculate that optimal DNA concentration may be the more important parameter related specifically to the introduction of DNA into individual zygotes; whereas, guide activity may prove to be the more important factor for promoting frequent deletion formation and efficient HR once donor DNA has entered the cell. Experimentation, performed in large numbers of cells, in vitro, and further optimization, in vivo, are likely to be productive avenues for further research and refinement of this technique.
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The authors thank the staff of The Jackson Laboratory’s Scientific Research Services in both the Genetic Engineering Technologies and Reproductive Sciences groups. The authors thank Dr. Narayanan Raghupathy, The Jackson Laboratory, for assistance with statistical analyses. The authors thank Jennifer Cook and Louise Dionne for mouse colony management and Judy Morgan for logistical support, as well as Rachel Urban, Susan Kales, and Jiayuan Shi for their molecular biological expertise. The authors thank Petra Klous, Bastiaan Bijl, and Erik Splinter of Cergentis, B.V., for their assistance with TLA analysis. Research reported in this publication was partially supported by the United States National Cancer Institute (http://www.cancer.gov) (award number P30CA034196) and by the Singapore Ministry of Health’s National Medical Research Council (http://www.nmrc.gov.sg) under its Clinician Scientist Award (NMRC/CSA/0051/2013), and Clinician Scientists Individual Research Grant (NMRC/CIRG/1330/2012), administered by the Singapore Ministry of Health’s National Medical Research Council. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript. The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institutes of Health (NIH) or the National Medical Research Council (Singapore).
The authors declare no competing interests.
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Leidy-Davis, T., Cheng, K., Goodwin, L.O. et al. Viable Mice with Extensive Gene Humanization (25-kbp) Created Using Embryonic Stem Cell/Blastocyst and CRISPR/Zygote Injection Approaches. Sci Rep 8, 15028 (2018). https://doi.org/10.1038/s41598-018-33408-9
- Clustered Regularly Interspaced Short Palindromic Repeat (CRISPR)
- Bcl-l Locus
- Cas9 mRNA
- Zygote Injection
- CRISPR Technology
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