We thank Saki Nishioka in Osaka University, Biotechnology Research and Development (nonprofit organization), and Mio Kikuchi and Reiko Sakamoto in the Institute of Medical Science, The University of Tokyo, for their excellent technical assistance. This work was supported by: the Ministry of Education, Culture, Sports, Science and Technology (MEXT)/Japan Society for the Promotion of Science (JSPS) KAKENHI grants to MI (JP19H05750, JP21H05033), and MO (20H03162); the Core Research for Evolutional Science and Technology (CREST), Japan Science and Technology Agency (JST) grant to MI (JPMJCR21N1 ); the Eunice Kennedy Shriver National Institute of Child Health and Human Development to MI (R01HD088412); the Bill &#38; Melinda Gates Foundation to MI (Grand Challenges Explorations grant INV-001902); and the Grant for Joint Research Project of the Research Institute for Microbial Diseases, Osaka University to MI, and MO.

All mouse experiments were approved by the Institutional Animal Care and Use Committee of the University of Tokyo (approval number PA17-63) and Osaka University (approval number Biken-AP-H30-01) and performed according to their guidelines as well as the ARRIVE guidelines (https://arriveguidelines.org).
1. Targeting vector construction
<ol>
	<li>Amplify a KI cassette (CreERT here, template DNA for the PCR is originally from a commercial gene synthesis company) and an approximate 1 kb fragment of 5&#39;- or 3&#39;-homology arms by PCR. For DNA cloning (step 1.3), add 15-mer overlap sequences at the 5&#39; end of each PCR primer. Purify the PCR DNA fragments by agarose gel electrophoresis, followed by extraction of the DNA fragment using a DNA purification kit.</li>
	<li>Linearize the backbone plasmid (e.g., pUC19 or pBS) using an appropriate restriction enzyme(s) that uniquely digests somewhere in the multi-cloning site for cloning. Then, purify the digested plasmid using a DNA purification kit.</li>
	<li>Clone each PCR fragment (e.g., 5&#39;-homology arm, 3&#39;-homology arm) and KI sequence simultaneously into the digested plasmid using a DNA cloning kit according to the manufacturer&#39;s instructions.</li>
	<li>Transform the competent cells using the constructed plasmid (step 1.3) by heating at 42 &#176;C for 1 min in a water bath, then seed them on an LB plate containing the appropriate concentration of antibiotics such as ampicillin or kanamycin. Culture them overnight for resistant clone selections.</li>
	<li>Pick up several (four to eight) individual colonies using 200 &#181;L pipette tips and transfer the tips into 3 mL of liquid LB containing appropriate antibiotics (100 &#181;g/mL ampicillin or 20 &#181;L/mL kanamycin) and culture overnight at 37 &#176;C with shaking.</li>
	<li>Purify the plasmid the following day using an endotoxin-free grade commercial plasmid purification kit according to the manufacturer&#39;s instructions. Confirm the cloned sequence in the plasmid by Sanger sequencing. Adjust the plasmid concentration at 1 &#181;g DNA/&#181;L using nuclease-free water. Use the plasmid as the gene targeting vector.</li>
</ol>
2. Preparation of the mouse embryonic fibroblast (MEF) as feeder cells for ESC
<ol>
	<li>Sacrifice 8-10-week-old pregnant ICR female mice (14.5 days postcoitum) by cervical dislocation. Wipe the abdomen well by using 70% (v/v) ethanol for sterilization, cut the abdomen using orbital scissors and forceps, and recover the fetus-containing uterus.</li>
	<li>Place the uterus into a 100 mm dish containing 10 mL of phosphate bovine serum (PBS) containing 100 U/mL penicillin and 100 &#181;g/mL streptomycin. Remove the placentas and extraembryonic tissues from the fetuses using orbital scissors and forceps. Mince the fetuses using orbital scissors and transfer the PBS solution containing the minced fetal cells to a 50 mL conical tube.</li>
	<li>Centrifuge at 280 x g for 5 min at 4 &#176;C and discard the supernatant by aspiration. Add 10 mL of 0.25% (w/v) trypsin-EDTA solution, mix well by pipetting, and then incubate for 10 min at 37 &#176;C using a water bath for trypsin digestion.</li>
	<li>Add 20 mL of MEF medium (DMEM containing 10% (v/v) fetal bovine serum, 100 U/mL penicillin, and 100 &#181;g/mL streptomycin) to stop the enzymatic reaction, mix well by gentle inversion, and centrifuge at 280 x g for 5 min at 4 &#176;C. Discard the supernatant by aspiration, add 10 mL of MEF medium, and mix well by pipetting.</li>
	<li>Seed the cell suspension in several new 100 mm dishes (prepare the same number of dishes as the number of fetuses with 10 mL of MEF medium for one 100 mm dish). Change the medium 4 to 5 h post-seeding to remove unattached cells and let the attached MEF grow. Passage the cells when they reach ~80% confluency using trypsin.</li>
	<li>Place the culture dishes containing the proliferating MEF in MEF medium, approximately 12-15 days post-seeding, in an X-ray irradiating device. Expose the MEF with a 50 Gy X-ray (total) to halt the cell cycle according to the manufacturer&#39;s instruction.</li>
	<li>Trypsinize the irradiated MEF by adding 2 mL of 0.25% trypsin-EDTA for one 100 mm dish for 5 min at 37 &#176;C, then add 4 mL of MEF medium to stop trypsin digestion and collect the cell suspension in a new 50 mL tube.</li>
	<li>Wash the MEF with a fresh MEF medium by centrifugation at 280 x g for 5 min at 4 &#176;C, count the number of cells using a cell counter with trypan blue staining, and freeze them at 1.6 x 106 cells/tube in a cell-freezing medium. Store until use; cells can be stably stored in liquid nitrogen for several years.</li>
</ol>
3. Cas9-RNP-DNA mixture preparation
<ol>
	<li>Dissolve tracrRNA and crisprRNA in dilution buffer (each RNA concentration at 200 &#181;M) by pipetting. Mix the tracrRNA solution, crisprRNA solution, and dilution buffer (volume ratio at 2:2:5) by gentle tapping and anneal each RNA using a thermal cycler at 95 &#176;C for 10 min followed by 1 &#176;C/min stepdown cycles until the temperature reaches 4 &#176;C. 
	NOTE: The gRNA sequence was designed using CRISPOR,&#160;http://crispor.tefor.net.</li>
	<li>Incubate the annealed RNAs, 10 &#181;g/&#181;L Cas9 nuclease, and the electroporation buffer mixed in a volume ratio of 5:3:2 at 37 &#176;C for 20 min to form the Cas9-RNP complex. In routine work, mix, and incubate 1.25 &#181;L of annealed RNA, 0.75 &#181;L of Cas9 nuclease, and 0.5 &#181;L of the electroporation buffer for one locus genome editing.</li>
	<li>Mix the following materials in a 1.5 mL tube: 10 &#181;L of electroporation buffer, 1 &#181;L of Cas9-RNP complex (step 3.2), and 1 &#181;L of circular targeting vector (1 &#181;g/&#181;L, step 1.6). The total amount of Cas9-RNP-DNA mixture is 12 &#181;L. Keep the Cas9-RNP-DNA mixture on ice until electroporation. 
	&#8203;NOTE: To prevent re-cleavage of the gRNA after KI, design the gRNA in a position where the gRNA recognition sequence is split by the integration of the KI donor. If the gRNA cannot be designed in such a location, several nucleotide silent mutations, by which the amino acid sequence does not change, are included in the plasmid of the KI donor.</li>
</ol>
4. Gene targeting of ESCs
<ol>
	<li>To prepare the gelatin-coated cell culture dishes, add 0.1% (w/v) gelatin solution at 2 mL for a 60 mm dish, 500 &#181;L for a 24-well plate, 100 &#181;L for a 96-well plate, and incubate for 2 h in a humid incubator. Remove the gelatin solution, wash twice with the same amount of PBS, and store at room temperature until use.</li>
	<li>Thaw mitotically inactivated frozen MEF stock (step 2.2) using a 37 &#176;C water bath for 1 min, and place the MEF on a gelatin-coated 60 mm dish (one frozen stock tube of MEF containing 1.6 x 106 cells for two 60 mm dishes, step 2.2) 1 day before ESC seeding.</li>
	<li>Thaw a frozen ESC stock tube (stored at 2 x 105 ESCs/tube; cell counting was carried out using a cell counter) using a 37 &#176;C water bath for 1 min, and place 1 x 105 ESCs onto a 60 mm dish containing pre-seeded MEF (step 4.1).</li>
	<li>Culture in 4 mL ESC culture medium (ESCM, DMEM-based modified medium with 15% (v/v) fetal bovine serum, 2 mM L-glutamine substrate, 100 U/mL penicillin, 100 &#181;g/mL streptomycin, 0.1 mM 2-mercaptoethanol, leukemia inhibitory factor, and t2i (0.2 &#181;M PD0325901 and 3 &#181;M CHIR99021) which maintains pluripotency of ESC11) at 37 &#176;C with 5% CO2 until the ESC reaches 50% to 70% confluency. 
	NOTE: We use three different lines of ESC: JM8.A3 from B6N, V6.5 from B6-129 F1, and in-house developed BALB/c ESC. The same KI protocols in this manuscript are used for all ESC lines.</li>
	<li>Wash the culturing ESC with 4 mL of PBS, then treat with 800 &#181;L of 0.25% trypsin-EDTA solution for 5 min at 37 &#176;C for digestion. Add 1 mL of ESCM to inactivate the trypsin and dissociate the ESCs to single cells by pipetting.</li>
	<li>Centrifuge the ESC-containing solution for 5 min at 280 x g, discard the supernatant, resuspend ESCs in fresh 1 mL of ESCM, and count the number of cells using a cell counter with trypan blue staining. Transfer 1 x 105 ESCs to a new 1.5 mL tube and wash them three times with PBS by centrifugation at 500 x g, 4 &#176;C.</li>
	<li>Resuspend the ESC pellet in 12 &#181;L of Cas9-RNP-DNA mixture (step 3.3) and mix well by gentle pipetting to avoid bubbling. Serve the resuspended ESC for electroporation. The electroporation system uses a single pulse at 1,400 V and 30 ms for Cas9-RNP-DNA transduction (Figure 1).</li>
	<li>Culture the electroporated ESCs in a 60 mm dish containing 4 mL of ESCM with mitotically inactivated MEF (section 4.2). Change the medium every day.</li>
	<li>Wash the ESCs with 4 mL of PBS 3 to 5 days after the electroporation, then treat with 800 &#181;L of 0.25% trypsin-EDTA and culture at 37 &#176;C for 5 min in a humid incubator for digestion. Add 2 mL of ESCM to stop the trypsin digestion and centrifuge the cell mixture at 280 x g for 5 min.</li>
	<li>Discard the supernatant, resuspend the ESCs in 1 mL of fresh ESCM, and count the cell concentration using a cell counter with trypan blue staining. Passage the ESCs at 1 x 103 ESCs per 60 mm dish containing ESCM and feeder MEF. Change the medium every day until the colony picks-up. 
	&#8203;NOTE: The reason why the ESC is passed once before pick-up was that genome editing may continue to occur after ESC division, so the first colony is not always the clone in many cases. Therefore, the first passage of ESC before the colony pick-up is an essential step to pick-up single clones.</li>
</ol>
5. PCR genotyping of targeted ESCs
<ol>
	<li>Aspirate ESCM from the ESC culture dish 5 to 7 days after the first passage (step 4.9) and add 4 mL of PBS. Pick up single ESC colonies with 5 &#181;L of PBS using a 20 &#181;L pipette under a stereomicroscope (30x to 40x magnification). Place the individual colonies in a well of a round-bottom 96-well plate containing 15 &#181;L of 0.25% trypsin-EDTA solution.</li>
	<li>Keep the 96-well plate on ice until 48 individual colonies are picked-up. Incubate the 96-well plate for 5 min in a 37 &#176;C humid 5% CO2 incubator, then add 80 &#181;L of ESCM to stop trypsin digestion and dissociate ESC colonies into single cells by pipetting. 
	NOTE: Since the KI efficiency of this method is usually 10%-50%, we routinely pick up 48 clones and first perform genotyping using 24 of them. If multiple KI clones cannot be obtained at this point, we further screen for KI using the remaining 24 clones.</li>
	<li>Transfer 40 &#181;L of ESC suspension (step 5) to a gelatin-coated feeder-free 96-well plate containing 50 &#181;L of ESCM per well for PCR genotyping. Transfer the remaining 60 &#181;L of ESC suspension into a well in a gelatin-coated 24-well plate, which contains 500 &#181;L of ESCM and feeder MEF, to make the frozen ESC stock.</li>
	<li>Stock individual ESC clones cultured in the 24-well plate (step 5.3) until they will reach 60% to 80% confluency. Recover individual ESC clones by trypsinization as mentioned above, collect cells in a new 1.5 mL tube, and centrifuge at 280 x g for 5 min. Discard the supernatant, resuspend the cells in 500 &#181;L of cell freezing medium, and freeze them using a -80 &#176;C deep freezer.</li>
	<li>For PCR genotyping, culture ESC clones in the 96-well feeder-free plate (step 5.3) until the ESC reaches more than 90% confluency. Remove ESCM from each well by aspiration and wash twice with 100 &#181;L of PBS.</li>
	<li>Aspirate the PBS and add 100 &#181;L of lysis buffer containing proteinase K, mix well, and transfer the ESC lysate to a new 1.5 mL tube. Heat the ESC lysate at 65 &#176;C for at least 1 h using a heat chamber. Extract and purify the genomic DNA using a conventional phenol-chloroform DNA purification method followed by ethanol precipitation.</li>
	<li>Dissolve the precipitated DNA in 20 &#181;L of DNase-free water and determine the purity and concentration of DNA using a spectrophotometer. Perform genomic PCR using locus-specific primer sets to amplify the target region. Then, check the sequence and choose the ESC clones with the desired KI sequences.</li>
</ol>
6. Preparation of eight-cell stage embryo and microinjection of ESCs
<ol>
	<li>Inject 5 IU of pregnant mare serum gonadotrophin (PMSG) intraperitoneally into adult ICR females. After 48 h, inject 5 IU of human chorionic gonadotrophin (hCG) into the same females, then mate the hormone-treated females with the ICR males. Check the copulatory plug in the vagina the following day (embryonic day 0.5, ED0.5). 
	NOTE: To evaluate chimerism by coat color ratios, use blastocyst from the ICR strain as a recipient for a ESC that has black or agouti coat color background, or blastocyst from the C57BL/6 strain as a recipient for a ESC that has the albino background.</li>
	<li>Collect the oviduct at ED1.5 and place it in HEPES buffered medium (FHM) drops. Recover the two-cell or four-cell stage embryos by flushing the oviduct with FHM using a flushing needle inserted into the infundibulum.</li>
	<li>Wash the collected embryos by moving them into several fresh FHM drops using a mouth pipette. Culture the embryos in 50 &#181;L of KSOM drop on a 35 mm cell culture dish covered with mineral oil at 37 &#176;C, 5% CO2 incubator for 1 day until the eight-cell or morula stage (ED2.5) is reached.</li>
	<li>If the embryos are not used on the next collection day, freeze them by vitrification according to the CARD protocol (http://card.medic.kumamoto-u.ac.jp/card/english/sigen/manual/ebvitri.html), and store them in liquid nitrogen until use.</li>
	<li>Prepare glass pipettes for holding the embryos (80-100 &#181;m outer diameter) and ESC injection (about 13 &#181;m diameter) using a puller and microforge.</li>
	<li>Integrate a holding pipette that contains FHM into a capillary holder connected to a microinjector and set up on the left side of the micromanipulator. Connect an injection pipette to another microinjector and set it up on the right side. Align the two pipettes straight in the field of the view of microscope.</li>
	<li>Dispense 5 &#181;L drops of 12% (w/v) polyvinylpyrrolidone (PVP) in FHM medium and 5 &#181;L drops of FHM onto the same lid of a 60 mm dish side-by-side and cover the drops with mineral oil. Transfer embryos in the 5 &#181;L FHM drop and add 1-5 &#181;L of the ESC suspension to the FHM drop that contains embryos. 
	NOTE: Leave the ESC and MEF suspension for 30 min in the 4 mL ESM on 60mm culture dish before the drop preparation. Since MEFs stick to the bottom faster than ESCs, this 30-minute incubation allows for the concentration of unattached ES cells in the supernatant.</li>
	<li>Wash inside the injection pipette with PVP, then move to the drop containing the embryos and ESCs.</li>
	<li>Pick up three individual ECS doublets that have just finished their cell division (six cells) in the injection pipette. Hold an eight-cell or morula stage embryo, which has completed compaction, with the holding pipette by aspiration. Make a hole in the zona pellucida with a piezoelectric pulse (intensity: 3; speed: 3). Expel the six-celled ESC inside the zona pellucida and pull the pipette out of the embryos.</li>
	<li>Wash the ESC-injected embryos with several KSOM drops gently using a mouth pipette and incubate them in a new 50 &#181;L KSOM drop covered with mineral oil at 37 &#176;C, 5% CO2 until the embryos develop to the blastocyst stage.</li>
	<li>Transfer the 10 ESC-injected blastocysts into each uterine horn of pseudopregnant female mice (2.5 days postcoitum, 20 blastocysts per head).</li>
	<li>After the surrogate mother has given birth, select at least two male chimeras with the highest chimerism ratio (70% or higher as confirmed by coat color), and then mate them with appropriate strain females to obtain F1 heterozygous KI.</li>
	<li>Breed individual KI mice with appropriate partners to obtain mice with desirable genotype(s) or genetic backgrounds suitable for research.</li>
</ol>

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The authors have no competing interests to disclose.

Gene targeting of ESCs followed by chimera production has been conventionally used for developing gene-manipulated mice. Nevertheless, gene knock-in efficiency remains low even though the targeting vector contains long (&#62; several kb in usual) homology arms with positive or negative drug selection gene cassettes. Our protocol introduced a tuned-up ESC KI method of long exogenous DNA using a circular plasmid without any drug selection cassettes as a targeting vector accompanied by Cas9-RNP-mediated genome editing at an acceptable efficiency for routine works. Thus, this protocol could help to substantially reduce the amount of time taken in producing genetically modified chimeric mice compared with the conventional ESC targeting.
In this protocol, we used CRISPR/Cas9-RNP to induce site-specific double-strand breaks in the genome, and a circular plasmid was used as the targeting vector instead of a linearized one. Linearized plasmids are conventionally used as a targeting vector for gene KI because of their increased efficiency of genomic integration8,9,10. However, many genomic integrations are nonspecific even though the vector contains homologous arms9. On the other hand, circular plasmids are rarely used as targeting vectors because of their hard-to-integrate feature into the genome of ESCs12 or fibroblasts13. Thus, it would be possible that applying a circular plasmid as a targeting vector accompanied by CRISPR/Cas9-mediated genome editing minimizes nonspecific random integration but maximizes the site-specific integration into the ESC genome. It would be notable that the induction efficiency of the double-strand break by CRISPR/Cas9 is quite important14, thus it would be essential to use gRNA which induces a double-strand break at high efficiency. It should be considered to re-design gRNA when the KI efficiency is too low. In the case shown in Figure 2, 40.9% of ESC clones showed a KI-specific band. In fact, as the core lab of the institute, we routinely perform gene targeting using ESCs by the method described here and have achieved KI efficiencies of 10%-50% for 1-2 kb sequences such as Cre, CreERT, or fluorescent reporters, although there are some variations depending on the gene locus. The longest DNA sequences we have successfully KI using this method is about 11.2 kb into the Rosa26 locus, and the efficiency was 12.2% (five KI colonies out of 41 analyzed colonies).
It would also be of note that this protocol uses eight-cell or morula stage embryos as recipients for ESC microinjection but not blastocyst stage embryos. Although we have not conducted comparing experiments in this paper, several reports have shown that injection of ESCs into eight-cell or morula stage embryos significantly improves the efficiency of ESC contribution to chimeric offspring compared to the ESC injection into blastocysts15,16,17,18. Indeed, ESC injections of various ESC lines, including C57BL/6, B6-129 F1, and BALB/c, commonly resulted in high coat color chimera development in some, but not all, offspring (see Figure 4). The limitation of the method is that the ESCs injected into the preimplantation embryo could not always contribute to germ cells in a chimera19,20. Germline transmission of ESCs would depend on the quality of each ESC clone19. Therefore, it would be advantageous to develop multiple ESC clone lines as a backup for stable chimeric mouse production. In conclusion, the protocols presented here use simple targeting vectors which include only each homology arm and gene of interest for KI without any drug-resistant cassette. Therefore, the vector construction would be much easier, and the culture period could be shortened compared to the conventional ESC targeting technique. This would help in quickly and facilitatively producing various types of genetically modified mice for future analysis in life science.

Producing genetically modified mice and analyzing their phenotype enables us to understand specific gene functions in detail, in vivo. Numerous important findings have been uncovered using gene-modified animal models in the life science field. Furthermore, since the report of genome editing technology using CRISPR/Cas91, research using genetically modified mice has quickly spread to many laboratories2,3. Genome editing of mouse zygotes by CRISPR/Cas9 has achieved acceptable efficiency for developing short DNA modification, such as indel mutation-oriented gene knockout4, single nucleotide replacement, or short peptide-tag insertion using single-stranded oligonucleotides (ssODNs) as knock-in (KI) donors5. On the other hand, the KI of large DNA fragments into zygotes by genome editing remains at a low efficiency compared to the short-size DNA modification6,7. In addition, it is difficult to use mouse strains such as BALB/c, which is an important strain for specific research areas like immunology, for zygote-based genome editing because their preimplantation embryos are susceptible to in vitro manipulation.
Another way to develop genetically modified mouse models is to use the embryonic stem cell (ESC) targeting technique followed by ESC injection into the preimplantation embryo to produce chimeras8,9,10, which is still routinely used as a conventional method. Although the acquisition rate for obtaining accurate KI-ESC clones is not very high in conventional ESC targeting methods, ESC targeting offers some advantages compared to zygote genome editing, especially for long DNA KI. For example, the KI efficiency of long DNA fragments (&#62; several kb) into the zygote genome is less evident6,7, and many zygotes are needed to develop even one line of KI mouse, which is undesirable in the current perspective of animal experiments. In contrast to zygote genome editing, long DNA targeting to ESCs followed by chimera production needs significantly fewer embryos than zygote genome editing. Furthermore, even though the preimplantation embryos from BALB/c are susceptible to in vitro manipulation, their ESCs can be maintained and handled in vitro11 as other competent 129 or F1 background ESCs, therefore, applicable for chimera productions. However, even though a targeting vector contains 5&#39; and 3&#39; homologous arms and drug resistance gene cassettes for positive or negative selection, the conventional KI efficiency of ESCs is generally insufficient, because of the high frequency of random genomic integration8,10, Thus, an improved method with precise ESC targeting efficiency is required. Recently, we reported a tuned-up ESC KI method using CRISPR/Cas9-based genome editing to achieve higher KI efficiency than conventional targeting methods11. The method we describe here is based on this procedure which enables long DNA (&#62; several to 10 kb) KI to ESCs with acceptable efficiency for routine works without drug selection; thus, the vector construction procedure would be much easier and need a shorter period, or the cell culture period would also become significantly shorter.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>BALB/c ESC</td>
			<td>-</td>
			<td>-</td>
			<td>ESC developed from BALB/c strain</td>
		</tr>
		<tr>
			<td>Bambanker</td>
			<td>Nippon Genetics</td>
			<td>CS-02-001</td>
			<td>Cell-freezeing medium. Section 2.6 and elsewhere</td>
		</tr>
		<tr>
			<td>Cas9 Nuclease V3</td>
			<td>IDT</td>
			<td>1081059</td>
			<td>Section 3.2 and elsewhere.</td>
		</tr>
		<tr>
			<td>CHIR99021</td>
			<td>FUJIFILM Wako</td>
			<td>038-23101</td>
			<td>Section 4.3</td>
		</tr>
		<tr>
			<td>CreERT gene fragment</td>
			<td>GeneWiz</td>
			<td></td>
			<td>Section 1.1.</td>
		</tr>
		<tr>
			<td>CRISPR-Cas9 crisprRNA</td>
			<td>IDT</td>
			<td></td>
			<td>crisprRNA. Section 3.1 and elsewhere.</td>
		</tr>
		<tr>
			<td>CRISPR-Cas9 tracrRNA</td>
			<td>IDT</td>
			<td>1072534</td>
			<td>tracrRNA. Section 3.1 and elsewhere.</td>
		</tr>
		<tr>
			<td>DMEM</td>
			<td>Nacalai</td>
			<td>08458-45</td>
			<td>MEF medium. Section 2.3 and elsewhere</td>
		</tr>
		<tr>
			<td>Duplex buffer</td>
			<td>IDT</td>
			<td>1072534</td>
			<td>RNA dilution buffer. Section 3.1 and elsewhere.</td>
		</tr>
		<tr>
			<td>FastGene Gel/PCR Extraction Kit</td>
			<td>Nippon Genetics</td>
			<td>FG-91302</td>
			<td>Section 1.1 and 1.2.</td>
		</tr>
		<tr>
			<td>GlutaMax</td>
			<td>Thermo Fisher</td>
			<td>35-050-061</td>
			<td>L-glutatime substrate</td>
		</tr>
		<tr>
			<td>hCG</td>
			<td>ASKA Animal Health</td>
			<td></td>
			<td>Section 6.1.</td>
		</tr>
		<tr>
			<td>In-Fusion HD Cloning Kit</td>
			<td>Clontech</td>
			<td>639648</td>
			<td>DNA cloning kit. Section 1.3 and elsewhere</td>
		</tr>
		<tr>
			<td>JM8.A3 ESC</td>
			<td>EuMMCR</td>
			<td>-</td>
			<td>ESC developed from C57BL/6N strain</td>
		</tr>
		<tr>
			<td>Knock-out DMEM</td>
			<td>Thermo Fisher</td>
			<td>10829018</td>
			<td>Section 4.3 and elsewhere, DMEM-based modified commercial medium.</td>
		</tr>
		<tr>
			<td>KSOM</td>
			<td>Merck</td>
			<td>MR-121-D</td>
			<td>Section 6.3 and 6.9.</td>
		</tr>
		<tr>
			<td>Leukemia inhibitory factor</td>
			<td>FUJIFILM Wako</td>
			<td>125-05603</td>
			<td>Section 4.3. No unit concentration data is supplied by the provider. Used 1,000-fold dilution in this protocol.</td>
		</tr>
		<tr>
			<td>Neon Electroporation system</td>
			<td>Thermo Fisher</td>
			<td>MPK5000</td>
			<td>Section 3.2, 4.5 and elsewhere. The system containes electroporation buffer as well used in section 3.2.</td>
		</tr>
		<tr>
			<td>NucleoSpin Plasmid Transfection-grade</td>
			<td>Takara</td>
			<td>U0490B</td>
			<td>Section 1.6.</td>
		</tr>
		<tr>
			<td>PD0325901</td>
			<td>FUJIFILM Wako</td>
			<td>162-25291</td>
			<td>Section 4.3</td>
		</tr>
		<tr>
			<td>PMSG</td>
			<td>ASKA Animal Health</td>
			<td></td>
			<td>Section 6.1.</td>
		</tr>
		<tr>
			<td>Tail lysis buffer</td>
			<td>Nacalai</td>
			<td>06169-95</td>
			<td>Section 5.5.</td>
		</tr>
		<tr>
			<td>Trypsin-EDTA</td>
			<td>Nacalai</td>
			<td>32777-15</td>
			<td>Section 2.2 and elsewhere</td>
		</tr>
		<tr>
			<td>V6.5 ESC</td>
			<td>-</td>
			<td>-</td>
			<td>ESC developed from B6J-129 F1 strain</td>
		</tr>
		<tr>
			<td>X-ray irradiation device</td>
			<td>Hitachi</td>
			<td>MBR-1618R-BE</td>
			<td>Section 2.6.</td>
		</tr>
	</tbody>
</table>

crispr/cas9-mediated highly efficient gene targeting in embryonic stem cells for developing gene-manipulated mouse models

The CRISPR/Cas9 system has made it possible to develop genetically modified mice by direct genome editing using fertilized zygotes. However, although the efficiency in developing gene-knockout mice by inducing small indel mutation would be sufficient enough, the efficiency of embryo genome editing for making large-size DNA knock-in (KI) is still low. Therefore, in contrast to the direct KI method in embryos, gene targeting using embryonic stem cells (ESCs) followed by embryo injection to develop chimera mice still has several advantages (e.g., high throughput targeting in vitro, multi-allele manipulation, and Cre and flox gene manipulation can be carried out in a short period). In addition, strains with difficult-to-handle embryos in vitro, such as BALB/c, can also be used for ESC targeting. This protocol describes the optimized method for large-size DNA (several kb) KI in ESCs by applying CRISPR/Cas9-mediated genome editing followed by chimera mice production to develop gene-manipulated mouse models.

We have targeted specific gene(s) in the ESC followed by chimera production to develop gene-manipulated mouse production according to our previous manuscript11. ESC genotyping (described in section 4) is routinely carried out by PCR using primers. The primers are designed on genomic sequences outside the homology arms and the specific sequences in the KI DNA fragment (Figure 2A). In that case, no wild-type allele is amplified, whereas a PCR amplicon of a specific size is detected only when the targeted exogenous DNA is KI at the target locus. Representative genotyping PCR results are shown in Figure 2B. Nine out of 22 clones (40.9%) showed a KI-specific band in this case. Three representative targeting results, including the result shown in Figure 2, are shown in Table 1. These results indicate that the method shown here is efficient and reproducible for gene KI without any drug selections.
ESC is picked up in an injection pipette, then a hole in the zona pellucida is made using a piezoelectric plus, and the ESC is released between the embryonic cells (Figure 3). Technically, this protocol to inject an ESC into an eight-cell or morula stage embryo is similar to the protocol for ESC injection into a blastocyst commonly used in many mouse facilities. Representative chimeric mice are shown in Figure 4. For coat color evaluation of chimerism, the embryo from the ICR strain (albino, white hair) was used as a recipient of B6 or B6-129 F1 ESC, and B6 embryos were used as a recipient of BALB/c ESCs (Figure 4).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/64385/64385fig01.jpg" /> 
Figure 1: A schematic of CRISPR/Cas9 ribonucleoprotein (RNP)-mediated circular plasmid integration into the specific locus of an ESC genome. Electroporation introduces a circular plasmid as a targeting vector into ESCs with Cas9-RNP. Abbreviations: GOI = gene of interest, HA = homology arm. <a href="https://www.jove.com/files/ftp_upload/64385/64385fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/64385/64385fig02.jpg" /> 
Figure 2: Genomic PCR analyses for KI screening of targeted ESC clones. (A) KI-specific PCR primers are designed on genomic sequences outside the homology arms (forward) and in the specific sequences in the KI DNA fragment (reverse). (B) Representative genotyping PCR results. A wild-type genome was used as a negative control. Abbreviations: GOI = gene of interest, HA = homology arm. <a href="https://www.jove.com/files/ftp_upload/64385/64385fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/64385/64385fig03.jpg" /> 
Figure 3: Representative images of eight-cell stage embryo injection. (A) For microinjection, three doublets of ESCs (six cells, arrowheads) are picked up. (B) A hole in the zona pellucida is made with a piezoelectric pulse, and ESCs are expelled in-between each blastomere. Scale bar shown is 50 &#181;m. <a href="https://www.jove.com/files/ftp_upload/64385/64385fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/64385/64385fig04.jpg" /> 
Figure 4: Representative images of chimera mice. (A,B) The ESC derived from C57BL/6N (JM8.A3, Agouti hair; A) or B6-129 F1 (Agouti hair; B) are injected into ICR (albino, white hair) embryos, followed by transferring the embryos to the mother surrogates. (C) The ESC derived from BALB/c (albino, white hair) is injected into C57BL/6J (black hair) embryos, followed by transferring the embryos to mother surrogates. <a href="https://www.jove.com/files/ftp_upload/64385/64385fig04large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Project ID</td>
			<td>Choromosome</td>
			<td>5&#39;HA length (bp)</td>
			<td>3&#39;HA length (bp)</td>
			<td>Insert size (bp)</td>
			<td>Number of analyzed clones</td>
			<td>Number of KI clones</td>
			<td>Efficiency (%)</td>
			<td>Remarks</td>
		</tr>
		<tr>
			<td>R26-CC*</td>
			<td>Chr6</td>
			<td>965</td>
			<td>1006</td>
			<td>5321</td>
			<td>23</td>
			<td>2</td>
			<td>8.7%</td>
			<td>-</td>
		</tr>
		<tr>
			<td>R4-03*</td>
			<td>Chr8</td>
			<td>1000</td>
			<td>997</td>
			<td>3070</td>
			<td>22</td>
			<td>6</td>
			<td>27.3%</td>
			<td>-</td>
		</tr>
		<tr>
			<td>P4-01*</td>
			<td>Chr15</td>
			<td>1000</td>
			<td>1000</td>
			<td>2569</td>
			<td>22</td>
			<td>9</td>
			<td>40.9%</td>
			<td>Shown in Figure 2</td>
		</tr>
	</tbody>
</table>
Table 1: KI efficiencies in three independent genomic loci in the ESC. *These projects have not been published so far. The name of these genes will be disclosed in independent manuscripts in the future.

Watch this Scientific Journal Video about CRISPR/Cas9-Mediated Highly Efficient Gene Targeting in Embryonic Stem Cells for Developing Gene-Manipulated Mouse Models at JoVE.com

CRISPR/Cas9-Mediated Highly Efficient Gene Targeting in Embryonic Stem Cells for Developing Gene-Manipulated Mouse Models

Here we present a protocol for developing genetically modified mouse models using embryonic stem cells, especially for large DNA knock-in (KI). This protocol is tuned up using CRISPR/Cas9 genome editing, resulting in significantly improved KI efficiency compared with the conventional homologous recombination-mediated linearized DNA targeting method.

The CRISPR/Cas9 system has made it possible to develop genetically modified mice by direct genome editing using fertilized zygotes. However, although the ...

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3.7K Views.  The University of Tokyo. Here we present a protocol for developing genetically modified mouse models using embryonic stem cells, especially for large DNA knock-in (KI). This protocol is tuned up using CRISPR/Cas9 genome editing, resulting in significantly improved KI efficiency compared with the conventional homologous recombination-mediated linearized DNA targeting method.

Video: CRISPR/Cas9-Mediated Highly Efficient Gene Targeting in Embryonic Stem Cells for Developing Gene-Manipulated Mouse Models

Neural Differentiation of Mouse Embryonic Stem Cells in Serum-free Monolayer Culture

The ability to differentiate mouse embryonic stem cells (ESC) to neural progenitors allows the study of the mechanisms controlling neural specification as well as the generation of mature neural cell types for further study. In this protocol we describe a method for the differentiation of ESC to neural progenitors using serum-free, monolayer culture. The method is scalable, efficient and results in production of ~70% neural progenitor cells within 4 - 6 days. It can be applied to ESC from various strains grown under a variety of conditions. Neural progenitors can be allowed to differentiate further into functional neurons and glia or analyzed by microscopy, flow cytometry or molecular techniques. The differentiation process is amenable to time-lapse microscopy and can be combined with the use of reporter lines to monitor the neural specification process. We provide detailed instructions on media preparation and cell density optimization to allow the process to be applied to most ESC lines and a variety of cell culture vessels.

This protocol describes in detail the method for generating neural progenitors from embryonic stem cells using a serum-free monolayer method. These progenitors can be used to derive mature neural cell types or to study the process of neural specification and is amenable to multiwell format scaling for compound screening.

The ability to differentiate mouse embryonic stem cells (ESC) to neural progenitors allows the study of the mechanisms controlling neural specification as ...

Protocols for Analyzing the Role of Paneth Cells in Regenerating the Murine Intestine using Conditional Cre-lox Mouse Models

The epithelial surface of the mammalian intestine is a dynamic tissue that renews every 3 - 7 days. Understanding this renewal process identified a population of rapidly cycling intestinal stem cells (ISCs) characterized by their expression of the Lgr5 gene. These are supported by a quiescent stem cell population, marked by Bmi-1 expression, capable of replacing them in the event of injury. Investigating the interactions between these populations is crucial to understanding their roles in disease and cancer. The ISCs exist within crypts on the intestinal surface, these niches support the ISC in replenishing the epithelia. The interaction between active and quiescent ISCs likely involves other differentiated cells within the niche, as it has previously been demonstrated that the &#8216;&#8216;stemness&#8217;&#8217; of the Lgr5 ISC is closely tied to the presence of their neighboring Paneth cells. Using conditional cre-lox mouse models we tested the effect of deleting the majority of active ISCs in the presence or absence of the Paneth cells. Here we describe the techniques and analysis undertaken to characterize the intestine and demonstrate that the Paneth cells play a crucial role within the ISC niche in aiding recovery following substantial insult.

Protocols for Analyzing the Role of Paneth Cells in Regenerating the Murine Intestine using Conditional Cre-lox Mouse Models

Intestinal epithelial stem cells (ISCs) are intermingled with Paneth cells. These cells are differentiated progeny of the ISC, which support the ISCs and provide antibacterial protection. Here we demonstrate how we used transgenic conditional mouse models to establish that Paneth cells play a crucial role in maintaining the intestinal epithelia.

The epithelial surface of the mammalian intestine is a dynamic tissue that renews every 3 - 7 days. Understanding this renewal process identified a ...

Generating CRISPR/Cas9 Mediated Monoallelic Deletions to Study Enhancer Function in Mouse Embryonic Stem Cells

Enhancers control cell identity by regulating tissue-specific gene expression in a position and orientation independent manner. These enhancers are often located distally from the regulated gene in intergenic regions or even within the body of another gene. The position independent nature of enhancer activity makes it difficult to match enhancers with the genes they regulate. Deletion of an enhancer region provides direct evidence for enhancer activity and is the gold standard to reveal an enhancer's role in endogenous gene transcription. Conventional homologous recombination based deletion methods have been surpassed by recent advances in genome editing technology which enable rapid and precisely located changes to the genomes of numerous model organisms. CRISPR/Cas9 mediated genome editing can be used to manipulate the genome in many cell types and organisms rapidly and cost effectively, due to the ease with which Cas9 can be targeted to the genome by a guide RNA from a bespoke expression plasmid. Homozygous deletion of essential gene regulatory elements might lead to lethality or alter cellular phenotype whereas monoallelic deletion of transcriptional enhancers allows for the study of cis-regulation of gene expression without this confounding issue. Presented here is a protocol for CRISPR/Cas9 mediated deletion in F1 mouse embryonic stem (ES) cells (Mus musculus129 x Mus castaneus). Monoallelic deletion, screening and expression analysis is facilitated by single nucleotide polymorphisms (SNP) between the two alleles which occur on average every 125 bp in these cells.

Experimental validation of enhancer activity is best approached by loss-of-function analysis. Presented here is an efficient protocol that uses CRISPR/Cas9 mediated deletion to study allele-specific regulation of gene transcription in F1 ES cells which contain a hybrid genome (Mus musculus129 x Mus castaneus).

Enhancers control cell identity by regulating tissue-specific gene expression in a position and orientation independent manner. These enhancers are often ...

A Quick and Efficient Method for the Purification of Endoderm Cells Generated from Human Embryonic Stem Cells

The differentiation capabilities of pluripotent stem cells such as embryonic stem cells (ESCs) allow a potential therapeutic application for cell replacement therapies. Terminally differentiated cell types could be used for the treatment of various degenerative diseases. In vitro differentiation of these cells towards tissues of the lung, liver and pancreas requires as a first step the generation of definitive endodermal cells. This step is rate-limiting for further differentiation towards terminally matured cell types such as insulin-producing beta cells, hepatocytes or other endoderm-derived cell types. Cells that are committed towards the endoderm lineage highly express a multitude of transcription factors such as FOXA2, SOX17, HNF1B, members of the GATA family, and the surface receptor CXCR4. However, differentiation protocols are rarely 100% efficient. Here, we describe a method for the purification of a CXCR4+ cell population after differentiation into the DE by using magnetic microbeads. This purification additionally removes cells of unwanted lineages. The gentle purification method is quick and reliable and might be used to improve downstream applications and differentiations.

Here, we describe a method for the purification of differentiated human embryonic stem cells that are committed towards the definitive endoderm for the improvement of downstream applications and further differentiations.

The differentiation capabilities of pluripotent stem cells such as embryonic stem cells (ESCs) allow a potential therapeutic application for cell ...

Structure-function Studies in Mouse Embryonic Stem Cells Using Recombinase-mediated Cassette Exchange

Gene engineering in mouse embryos or embryonic stem cells (mESCs) allows for the study of the function of a given protein. Proteins are the workhorses of the cell and often consist of multiple functional domains, which can be influenced by posttranslational modifications. The depletion of the entire protein in conditional or constitutive knock-out (KO) mice does not take into account this functional diversity and regulation. An mESC line and a derived mouse model, in which a docking site for FLPe recombination-mediated cassette exchange (RMCE) was inserted within the ROSA26 (R26) locus, was previously reported. Here, we report on a structure-function approach that allows for molecular dissection of the different functionalities of a multidomain protein. To this end, RMCE-compatible mice must be crossed with KO mice and then RMCE-compatible KO mESCs must be isolated. Next, a panel of putative rescue constructs can be introduced into the R26 locus via RMCE targeting. The candidate rescue cDNAs can be easily inserted between RMCE sites of the targeting vector using recombination cloning. Next, KO mESCs are transfected with the targeting vector in combination with an FLPe recombinase expression plasmid. RMCE reactivates the promoter-less neomycin-resistance gene in the ROSA26 docking sites and allows for the selection of the correct targeting event. In this way, high targeting efficiencies close to 100% are obtained, allowing for insertion of multiple putative rescue constructs in a semi-high throughput manner. Finally, a multitude of R26-driven rescue constructs can be tested for their ability to rescue the phenotype that was observed in parental KO mESCs. We present a proof-of-principle structure-function study in p120 catenin (p120ctn) KO mESCs using endoderm differentiation in embryoid bodies (EBs) as the phenotypic readout. This approach enables the identification of important domains, putative downstream pathways, and disease-relevant point mutations that underlie KO phenotypes for a given protein.

Proteins often contain multiple domains that can exert different cellular functions. Gene knock-outs (KO) do not consider this functional diversity. Here, we report a recombination-mediated cassette exchange (RMCE)-based structure-function approach in KO embryonic stem cells that allows for the molecular dissection of various functional domains or variants of a protein.

Gene engineering in mouse embryos or embryonic stem cells (mESCs) allows for the study of the function of a given protein. Proteins are the workhorses of ...

Live Imaging of Mouse Secondary Palate Fusion

The fusion of the secondary palatal shelves to form the intact secondary palate is a key process in mammalian development and its disruption can lead to cleft secondary palate, a common congenital anomaly in humans. Secondary palate fusion has been extensively studied leading to several proposed cellular mechanisms that may mediate this process. However, these studies have been mostly performed on fixed embryonic tissues at progressive timepoints during development or in fixed explant cultures analyzed at static timepoints. Static analysis is limited for the analysis of dynamic morphogenetic processes such a palate fusion and what types of dynamic cellular behaviors mediate palatal fusion is incompletely understood. Here we describe a protocol for live imaging of ex vivo secondary palate fusion in mouse embryos. To examine cellular behaviors of palate fusion, epithelial-specific Keratin14-cre was used to label palate epithelial cells in ROSA26-mTmGflox reporter embryos. To visualize filamentous actin, Lifeact-mRFPruby reporter mice were used. Live imaging of secondary palate fusion was performed by dissecting recently-adhered secondary palatal shelves of embryonic day (E) 14.5 stage embryos and culturing in agarose-containing media on a glass bottom dish to enable imaging with an inverted confocal microscope. Using this method, we have detected a variety of novel cellular behaviors during secondary palate fusion. An appreciation of how distinct cell behaviors are coordinated in space and time greatly contributes to our understanding of this dynamic morphogenetic process. This protocol can be applied to mutant mouse lines, or cultures treated with pharmacological inhibitors to further advance understanding of how secondary palate fusion is controlled.

Here, we present a protocol for live imaging of mouse secondary palate fusion using confocal microscopy. This protocol can be used in combination with a variety of fluorescent reporter mouse lines, and with pathway inhibitors for mechanistic insight. This protocol can be adapted for live imaging in other developmental systems.

The fusion of the secondary palatal shelves to form the intact secondary palate is a key process in mammalian development and its disruption can lead to ...

Single-cell Photoconversion in Living Intact Zebrafish

Animal and plant tissue is composed of distinct populations of cells. These cells interact over time to build and maintain the tissue and can cause disease when disrupted. Scientists have developed clever techniques to investigate characteristics and natural dynamics of these cells within intact tissue by expressing fluorescent proteins in subsets of cells. However, at times, experiments require more selected visualization of cells within the tissue, sometimes at the single-cell or population-of-cells manner. To achieve this and visualize single cells within a population of cells, scientists have utilized single-cell photoconversion of fluorescent proteins. To demonstrate this technique, we show here how to direct UV light to an Eos-expressing cell of interest in an intact, living zebrafish. We then image those photoconverted Eos+ cells 24 h later to determine how they changed in the tissue. We describe two techniques: single cell photoconversion and photoconversions of populations of cell. These techniques can be used to visualize cell-cell interactions, cell-fate and differentiation, and cell migrations, making it a technique that is applicable in numerous biological questions.

Here, we present a protocol to show how cell photoconversion is achieved through UV exposure to specific areas expressing the fluorescent protein, Eos, in living animals.

Animal and plant tissue is composed of distinct populations of cells. These cells interact over time to build and maintain the tissue and can cause ...

Identification of Skeletal Muscle Satellite Cells by Immunofluorescence with Pax7 and Laminin Antibodies

Immunofluorescence is an effective method that helps to identify different cell types on tissue sections. In order to study the desired cell population, antibodies for specific cell markers are applied on tissue sections. In adult skeletal muscle, satellite cells (SCs) are stem cells that contribute to muscle repair and regeneration. Therefore, it is important to visualize and trace the satellite cell population under different physiological conditions. In resting skeletal muscle, SCs reside between the basal lamina and myofiber plasma membrane. A commonly used marker for identifying SCs on the myofibers or in cell culture is the paired box protein Pax7. In this article, an optimized Pax7 immunofluorescence protocol on skeletal muscle sections is presented that minimizes non-specific staining and background. Another antibody that recognizes a protein (laminin) of the basal lamina was also added to help identify SCs. Similar protocols can also be used to perform double or triple labeling with Pax7 and antibodies for additional proteins of interest.

The precise identification of satellite cells is essential for studying their functions under various physiological and pathological conditions. This article presents a protocol to identify satellite cells on adult skeletal muscle sections by immunofluorescence-based staining.

Immunofluorescence is an effective method that helps to identify different cell types on tissue sections. In order to study the desired cell population, ...

Efficient Differentiation of Human Pluripotent Stem Cells into Liver Cells

The liver detoxifies harmful substances, secretes vital proteins, and executes key metabolic activities, thus sustaining life. Consequently, liver failure&#8212;which can be caused by chronic alcohol intake, hepatitis, acute poisoning, or other insults&#8212;is a severe condition that can culminate in bleeding, jaundice, coma, and eventually death. However, approaches to treat liver failure, as well as studies of liver function and disease, have been stymied in part by the lack of a plentiful supply of human liver cells. To this end, this protocol details the efficient differentiation of human pluripotent stem cells (hPSCs) into hepatocyte-like cells, guided by a developmental roadmap that describes how liver fate is specified across six consecutive differentiation steps. By manipulating developmental signaling pathways to promote liver differentiation and to explicitly suppress the formation of unwanted cell fates, this method efficiently generates populations of human liver bud progenitors and hepatocyte-like cells by days 6 and 18 of PSC differentiation, respectively. This is achieved through the temporally-precise control of developmental signaling pathways, exerted by small molecules and growth factors in a serum-free culture medium. Differentiation in this system occurs in monolayers and yields hepatocyte-like cells that express characteristic hepatocyte enzymes and have the ability to engraft a mouse model of chronic liver failure. The ability to efficiently generate large numbers of human liver cells in vitro has ramifications for treatment of liver failure, for drug screening, and for mechanistic studies of liver disease.

This protocol details a monolayer, serum-free method to efficiently generate hepatocyte-like cells from human pluripotent stem cells (hPSCs) in 18 days. This entails six steps as hPSCs sequentially differentiate into intermediate cell-types such as the primitive streak, definitive endoderm, posterior foregut and liver bud progenitors before forming hepatocyte-like cells.

The liver detoxifies harmful substances, secretes vital proteins, and executes key metabolic activities, thus sustaining life. Consequently, liver ...

In Vitro Generation of Somite Derivatives from Human Induced Pluripotent Stem Cells

In response to signals such as WNTs, bone morphogenetic proteins (BMPs), and sonic hedgehog (SHH) secreted from surrounding tissues, somites (SMs) give rise to multiple cell types, including the myotome (MYO), sclerotome (SCL), dermatome (D), and syndetome (SYN), which in turn develop into skeletal muscle, axial skeleton, dorsal dermis, and axial tendon/ligament, respectively. Therefore, the generation of SMs and their derivatives from human induced pluripotent stem cells (iPSCs) is critical to obtain pluripotent stem cells (PSCs) for application in regenerative medicine and for disease research in the field of orthopedic surgery. Although the induction protocols for MYO and SCL from PSCs have been previously reported by several researchers, no study has yet demonstrated the induction of SYN and D from iPSCs. Therefore, efficient induction of fully competent SMs remains a major challenge. Here, we recapitulate human SM patterning with human iPSCs in vitro by mimicking the signaling environment during chick/mouse SM development, and report on methods of systematic induction of SM derivatives (MYO, SCL, D, and SYN) from human iPSCs under chemically defined conditions through the presomitic mesoderm (PSM) and SM states. Knowledge regarding chick/mouse&#160;SM development was successfully applied to the induction of SMs with human iPSCs. This method could be a novel tool for studying human somitogenesis and patterning without the use of embryos and for cell-based therapy and disease modeling.

We present here a protocol for the differentiation of human induced pluripotent stem cells into each somite derivative (myotome, sclerotome, dermatome, and syndetome) in chemically defined conditions, which has applications in future disease modeling and cell-based therapies in orthopedic surgery.

In response to signals such as WNTs, bone morphogenetic proteins (BMPs), and sonic hedgehog (SHH) secreted from surrounding tissues, somites (SMs) give ...