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Liu Y, Liu S, Sheng H, Feng X, Wang S, Hu Y, Zhang L, Cai B, Ma Y. Revolutionizing cattle breeding: Gene editing advancements for enhancing economic traits. Gene 2024; 927:148595. [PMID: 38795857 DOI: 10.1016/j.gene.2024.148595] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/28/2024] [Revised: 05/15/2024] [Accepted: 05/20/2024] [Indexed: 05/28/2024]
Abstract
Beef and dairy products are rich in protein and amino acids, making them highly nutritious for human consumption. The increasing use of gene editing technology in agriculture has paved the way for genetic improvement in cattle breeding via the development of the CRISPR/Cas (clustered regularly interspaced short palindromic repeats/CRISPR-associated protein) system. Gene sequences are artificially altered and employed in the pursuit of improving bovine breeding research through targeted knockout, knock-in, substitution, and mutation methods. This review offers a comprehensive analysis of the advancements in gene editing technology and its diverse applications in enhancing both quantitative and qualitative traits across livestock. These applications encompass areas such as meat quality, milk quality, fertility, disease resistance, environmental adaptability, sex control, horn development, and coat colour. Furthermore, the review considers prospective ideas and insights that may be employed to refine breeding traits, enhance editing efficiency, and navigate the ethical considerations associated with these advancements. The review's focus on improving the quality of beef and milk is intended to enhance the economic viability of these products. Furthermore, it constitutes a valuable resource for scholars and researchers engaged in the fields of cattle genetic improvement and breeding.
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Affiliation(s)
- Yuan Liu
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Shuang Liu
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Hui Sheng
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Xue Feng
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Shuzhe Wang
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Yamei Hu
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Lingkai Zhang
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
| | - Bei Cai
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China
| | - Yun Ma
- College of Animal Science and Technology, Ningxia University, Yinchuan 750021, China; Key Laboratory of Ruminant Molecular and Cellular Breeding of Ningxia Hui Autonomous Region, Ningxia University, Yinchuan 750021, China.
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Yuan YG, Liu SZ, Farhab M, Lv MY, Zhang T, Cao SX. Genome editing: An insight into disease resistance, production efficiency, and biomedical applications in livestock. Funct Integr Genomics 2024; 24:81. [PMID: 38709433 DOI: 10.1007/s10142-024-01364-5] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/04/2024] [Revised: 04/29/2024] [Accepted: 05/01/2024] [Indexed: 05/07/2024]
Abstract
One of the primary concerns for the survival of the human species is the growing demand for food brought on by an increasing global population. New developments in genome-editing technology present promising opportunities for the growth of wholesome and prolific farm animals. Genome editing in large animals is used for a variety of purposes, including biotechnology to improve food production, animal health, and pest management, as well as the development of animal models for fundamental research and biomedicine. Genome editing entails modifying genetic material by removing, adding, or manipulating particular DNA sequences from a particular locus in a way that does not happen naturally. The three primary genome editors are CRISPR/Cas 9, TALENs, and ZFNs. Each of these enzymes is capable of precisely severing nuclear DNA at a predetermined location. One of the most effective inventions is base editing, which enables single base conversions without the requirement for a DNA double-strand break (DSB). As reliable methods for precise genome editing in studies involving animals, cytosine and adenine base editing are now well-established. Effective zygote editing with both cytosine and adenine base editors (ABE) has resulted in the production of animal models. Both base editors produced comparable outcomes for the precise editing of point mutations in somatic cells, advancing the field of gene therapy. This review focused on the principles, methods, recent developments, outstanding applications, the advantages and disadvantages of ZFNs, TALENs, and CRISPR/Cas9 base editors, and prime editing in diverse lab and farm animals. Additionally, we address the methodologies that can be used for gene regulation, base editing, and epigenetic alterations, as well as the significance of genome editing in animal models to better reflect real disease. We also look at methods designed to increase the effectiveness and precision of gene editing tools. Genome editing in large animals is used for a variety of purposes, including biotechnology to improve food production, animal health, and pest management, as well as the development of animal models for fundamental research and biomedicine. This review is an overview of the existing knowledge of the principles, methods, recent developments, outstanding applications, the advantages and disadvantages of zinc finger nucleases (ZFNs), transcription-activator-like endonucleases (TALENs), and clustered regularly interspaced short palindromic repeats associated protein 9 (CRISPR/Cas 9), base editors and prime editing in diverse lab and farm animals, which will offer better and healthier products for the entire human race.
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Affiliation(s)
- Yu-Guo Yuan
- College of Veterinary Medicine/Key Laboratory of Animal Genetic Engineering, Yangzhou University, Yangzhou, 225009, Jiangsu, China.
- Jiangsu Co-Innovation Center of Prevention and Control of Important Animal Infectious Diseases and Zoonoses, Yangzhou University, Yangzhou, 225009, Jiangsu, China.
| | - Song-Zi Liu
- College of Veterinary Medicine/Key Laboratory of Animal Genetic Engineering, Yangzhou University, Yangzhou, 225009, Jiangsu, China
- Jiangsu Co-Innovation Center of Prevention and Control of Important Animal Infectious Diseases and Zoonoses, Yangzhou University, Yangzhou, 225009, Jiangsu, China
| | - Muhammad Farhab
- College of Veterinary Medicine/Key Laboratory of Animal Genetic Engineering, Yangzhou University, Yangzhou, 225009, Jiangsu, China
- Jiangsu Co-Innovation Center of Prevention and Control of Important Animal Infectious Diseases and Zoonoses, Yangzhou University, Yangzhou, 225009, Jiangsu, China
| | - Mei-Yun Lv
- College of Veterinary Medicine/Key Laboratory of Animal Genetic Engineering, Yangzhou University, Yangzhou, 225009, Jiangsu, China
- Jiangsu Co-Innovation Center of Prevention and Control of Important Animal Infectious Diseases and Zoonoses, Yangzhou University, Yangzhou, 225009, Jiangsu, China
| | - Ting Zhang
- School of Animal Husbandry and Veterinary Medicine, Jiangsu Vocational College of Agriculture and Forestry, Jurong, 212499, China
| | - Shao-Xiao Cao
- Institute of Animal Science, Jiangsu Academy of Agricultural Sciences, Nanjing, 210014, China
- Jiangsu Provincial Engineering Research Center for Precision animal Breeding, Nanjing, 210014, China
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Navarro-Serna S, Piñeiro-Silva C, Fernández-Martín I, Dehesa-Etxebeste M, López de Munain A, Gadea J. Oocyte electroporation prior to in vitro fertilization is an efficient method to generate single, double, and multiple knockout porcine embryos of interest in biomedicine and animal production. Theriogenology 2024; 218:111-118. [PMID: 38320372 DOI: 10.1016/j.theriogenology.2024.01.040] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/14/2023] [Revised: 01/31/2024] [Accepted: 01/31/2024] [Indexed: 02/08/2024]
Abstract
Genetically modified pigs play a critical role in mimicking human diseases, xenotransplantation, and the development of pigs resistant to viral diseases. The use of programmable endonucleases, including the CRISPR/Cas9 system, has revolutionized the generation of genetically modified pigs. This study evaluates the efficiency of electroporation of oocytes prior to fertilization in generating edited gene embryos for different models. For single gene editing, phospholipase C zeta (PLC ζ) and fused in sarcoma (FUS) genes were used, and the concentration of sgRNA and Cas9 complexes was optimized. The results showed that increasing the concentration resulted in higher mutation rates without affecting the blastocyst rate. Electroporation produced double knockouts for the TPC1/TPC2 genes with high efficiency (79 %). In addition, resistance to viral diseases such as PRRS and swine influenza was achieved by electroporation, allowing the generation of double knockout embryo pigs (63 %). The study also demonstrated the potential for multiple gene editing in a single step using electroporation, which is relevant for xenotransplantation. The technique resulted in the simultaneous mutation of 5 genes (GGTA1, B4GALNT2, pseudo B4GALNT2, CMAH and GHR). Overall, electroporation proved to be an efficient and versatile method to generate genetically modified embryonic pigs, offering significant advances in biomedical and agricultural research, xenotransplantation, and disease resistance. Electroporation led to the processing of numerous oocytes in a single session using less expensive equipment. We confirmed the generation of gene-edited porcine embryos for single, double, or quintuple genes simultaneously without altering embryo development to the blastocyst stage. The results provide valuable insights into the optimization of gene editing protocols for different models, opening new avenues for research and applications in this field.
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Affiliation(s)
- Sergio Navarro-Serna
- Department Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain
| | - Celia Piñeiro-Silva
- Department Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain
| | - Irene Fernández-Martín
- Department Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain
| | | | - Adolfo López de Munain
- IIS Biodonostia, Neuroscience, San Sebastián, Spain; Department of Neurology. Hospital Universitario Donostia-OSAKIDETZA, San Sebastián, Spain; Department of Neurosciences. University of the Basque Country (UPV-EHU), San Sebastián, Spain; CIBERNED (CIBER), Institute Carlos III, Madrid, Spain
| | - Joaquín Gadea
- Department Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain.
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Piñeiro-Silva C, Gadea J. Optimizing oocyte electroporation for genetic modification of porcine embryos: Evaluation of the parthenogenetic activation. Theriogenology 2024; 218:126-136. [PMID: 38325149 DOI: 10.1016/j.theriogenology.2024.01.041] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/03/2023] [Revised: 01/31/2024] [Accepted: 01/31/2024] [Indexed: 02/09/2024]
Abstract
In reproductive biology, understanding the effects of novel techniques on early embryo development is of paramount importance. To date, the effects of electrical activation on oocytes prior to in vitro fertilization (IVF) are not well understood. The aim of this study was to investigate the effects of oocyte electroporation prior to IVF on embryo development and to differentiate between true embryos and parthenotes by using a TPCN2 knock-out (KO) male to evaluate the presence of the KO allele in the resulting blastocysts. The study consisted of three experiments. The first one examined oocyte electroporation with and without subsequent IVF and found that electroporated oocytes had higher activation rates, increased occurrence of a single pronucleus, and no effect on sperm penetration. Cleavage rates improved in electroporated oocytes, but blastocyst rates remained constant. Genotype analysis revealed a significant increase in the proportion of parthenotes in the electroporated groups compared to the IVF control (30.2 % vs. 6.8 %). The second experiment compared two electroporation media, Opti-MEM and Nuclease-Free Duplex Buffer (DB). DB induced higher oocyte degeneration rates, and lower cleavage and blastocyst rates than Opti-MEM, while parthenogenetic formation remained consistent (60.0 and 48.5 %). In the third experiment, the timing of electroporation relative to IVF was evaluated (1 h before IVF, immediately before IVF and 7 h after IVF). Electroporation immediately before IVF resulted in higher activation rates and different pronuclear proportions compared to the other timing groups. The penetration rate was higher in the immediate electroporation group, and cleavage rate improved in all electroporated groups compared to the control. Blastocyst rates remained constant. Genotyping revealed no significant differences in parthenote proportions among the timing groups, but these were higher than the control (56.25 %, 63.89 %, 51.61 %, 2.44 %, respectively), and showed higher mutation rates when electroporation was performed 7 h after IVF. Overall, this comprehensive study sheds light on the potential of electroporation for creating genetically modified embryos and the importance of media selection and timing in the process, the best media being the Opti-MEM and the more efficient timing regarding mutation rate, 7 h post-IVF, even when the parthenote formation did not differ among electroporated groups. Further studies are needed to reduce the parthenogenetic activation while maintaining high mutation rates to optimize the use of this procedure for the generation of gene-edited pig embryos by oocyte/zygote electroporation.
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Affiliation(s)
- Celia Piñeiro-Silva
- Department of Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain
| | - Joaquín Gadea
- Department of Physiology, University of Murcia, International Excellence Campus for Higher Education and Research "Campus Mare Nostrum" and Institute for Biomedical Research of Murcia (IMIB-Arrixaca), 30100, Murcia, Spain.
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5
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Biase FH, Schettini G. Protocol for the electroporation of CRISPR-Cas for DNA and RNA targeting in Bos taurus zygotes. STAR Protoc 2024; 5:102940. [PMID: 38460133 PMCID: PMC10941008 DOI: 10.1016/j.xpro.2024.102940] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/25/2023] [Revised: 01/09/2024] [Accepted: 02/21/2024] [Indexed: 03/11/2024] Open
Abstract
The use of CRISPR-Cas9 ribonucleoproteins has revolutionized manipulation of genomes. Here, we present a protocol for the electroporation of CRISPR-Cas for DNA and RNA targeting in Bos taurus zygotes. First, we describe steps for production and preparation of presumptive zygotes for electroporation. The first electroporation introduces ribonucleoproteins formed by Cas9D10A with two guide RNAs to target DNA, and the second introduces the same ribonucleoprotein complex to target DNA plus Cas13a with one guide RNA to target RNAs. For complete details on the use and execution of this protocol, please refer to Nix et al.1.
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Affiliation(s)
- Fernando H Biase
- Virginia Polytechnique Institute and State University, Blacksburg, VA 24061, USA.
| | - Gustavo Schettini
- Virginia Polytechnique Institute and State University, Blacksburg, VA 24061, USA
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Zheng Y, Li Y, Zhou K, Li T, VanDusen NJ, Hua Y. Precise genome-editing in human diseases: mechanisms, strategies and applications. Signal Transduct Target Ther 2024; 9:47. [PMID: 38409199 PMCID: PMC10897424 DOI: 10.1038/s41392-024-01750-2] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/17/2023] [Revised: 01/15/2024] [Accepted: 01/17/2024] [Indexed: 02/28/2024] Open
Abstract
Precise genome-editing platforms are versatile tools for generating specific, site-directed DNA insertions, deletions, and substitutions. The continuous enhancement of these tools has led to a revolution in the life sciences, which promises to deliver novel therapies for genetic disease. Precise genome-editing can be traced back to the 1950s with the discovery of DNA's double-helix and, after 70 years of development, has evolved from crude in vitro applications to a wide range of sophisticated capabilities, including in vivo applications. Nonetheless, precise genome-editing faces constraints such as modest efficiency, delivery challenges, and off-target effects. In this review, we explore precise genome-editing, with a focus on introduction of the landmark events in its history, various platforms, delivery systems, and applications. First, we discuss the landmark events in the history of precise genome-editing. Second, we describe the current state of precise genome-editing strategies and explain how these techniques offer unprecedented precision and versatility for modifying the human genome. Third, we introduce the current delivery systems used to deploy precise genome-editing components through DNA, RNA, and RNPs. Finally, we summarize the current applications of precise genome-editing in labeling endogenous genes, screening genetic variants, molecular recording, generating disease models, and gene therapy, including ex vivo therapy and in vivo therapy, and discuss potential future advances.
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Affiliation(s)
- Yanjiang Zheng
- Key Laboratory of Birth Defects and Related Diseases of Women and Children of MOE, Department of Pediatrics, West China Second University Hospital, Sichuan University, Chengdu, Sichuan, 610041, China
| | - Yifei Li
- Key Laboratory of Birth Defects and Related Diseases of Women and Children of MOE, Department of Pediatrics, West China Second University Hospital, Sichuan University, Chengdu, Sichuan, 610041, China
| | - Kaiyu Zhou
- Key Laboratory of Birth Defects and Related Diseases of Women and Children of MOE, Department of Pediatrics, West China Second University Hospital, Sichuan University, Chengdu, Sichuan, 610041, China
| | - Tiange Li
- Department of Cardiovascular Surgery, West China Hospital, Sichuan University, Chengdu, Sichuan, 610041, China
| | - Nathan J VanDusen
- Department of Pediatrics, Herman B Wells Center for Pediatric Research, Indiana University School of Medicine, Indianapolis, IN, 46202, USA.
| | - Yimin Hua
- Key Laboratory of Birth Defects and Related Diseases of Women and Children of MOE, Department of Pediatrics, West China Second University Hospital, Sichuan University, Chengdu, Sichuan, 610041, China.
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Punetha M, Kumar D, Saini S, Chaudhary S, Bajwa KK, Sharma S, Mangal M, Yadav PS, Green JA, Whitworth K, Datta TK. Optimising Electroporation Condition for CRISPR/Cas-Mediated Knockout in Zona-Intact Buffalo Zygotes. Animals (Basel) 2023; 14:134. [PMID: 38200865 PMCID: PMC10778295 DOI: 10.3390/ani14010134] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/23/2023] [Revised: 12/27/2023] [Accepted: 12/28/2023] [Indexed: 01/12/2024] Open
Abstract
Somatic cell nuclear transfer or cytoplasm microinjection has widely been used to produce genome-edited farm animals; however, these methods have several drawbacks which reduce their efficiency. In the present study, we describe an easy adaptable approach for the introduction of mutations using CRISPR-Cas9 electroporation of zygote (CRISPR-EP) in buffalo. The goal of the study was to determine the optimal conditions for an experimental method in which the CRISPR/Cas9 system is introduced into in vitro-produced buffalo zygotes by electroporation. Electroporation was performed using different combinations of voltage, pulse and time, and we observed that the electroporation in buffalo zygote at 20 V/mm, 5 pulses, 3 msec at 10 h post insemination (hpi) resulted in increased membrane permeability and higher knockout efficiency without altering embryonic developmental potential. Using the above parameters, we targeted buffalo POU5F1 gene as a proof of concept and found no variations in embryonic developmental competence at cleavage or blastocyst formation rate between control, POU5F1-KO, and electroporated control (EC) embryos. To elucidate the effect of POU5F1-KO on other pluripotent genes, we determined the relative expression of SOX2, NANOG, and GATA2 in the control (POU5F1 intact) and POU5F1-KO-confirmed blastocyst. POU5F1-KO significantly (p ≤ 0.05) altered the expression of SOX2, NANOG, and GATA2 in blastocyst stage embryos. In conclusion, we standardized an easy and straightforward protocol CRISPR-EP method that could be served as a useful method for studying the functional genomics of buffalo embryos.
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Affiliation(s)
- Meeti Punetha
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Dharmendra Kumar
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Sheetal Saini
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Suman Chaudhary
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Kamlesh Kumari Bajwa
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Surabhi Sharma
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Manu Mangal
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Prem S. Yadav
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
| | - Jonathan A. Green
- Division of Animal Sciences, University of Missouri, Columbia, MO 65211, USA
| | - Kristin Whitworth
- Division of Animal Sciences, University of Missouri, Columbia, MO 65211, USA
| | - Tirtha K. Datta
- Animal Physiology and Reproduction Division, ICAR-Central Institute for Research on Buffaloes, Hisar 125001, Haryana, India
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Jose B, Punetha M, Tripathi MK, Khanna S, Yadav V, Singh AK, Kumar B, Singh K, Chouhan VS, Sarkar M. CRISPR/Cas mediated disruption of BMPR-1B gene and introduction of FecB mutation into the Caprine embryos using Easi-CRISPR strategy. Theriogenology 2023; 211:125-133. [PMID: 37619525 DOI: 10.1016/j.theriogenology.2023.08.008] [Citation(s) in RCA: 1] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/07/2023] [Revised: 08/14/2023] [Accepted: 08/14/2023] [Indexed: 08/26/2023]
Abstract
Bone Morphogenetic Proteins play a significant role in ovarian physiology and contribute to the reproductive fitness of mammals. The BMPR-1B/FecB mutation, a loss of function mutation increases litter size by 1-2 with each number of mutated alleles in sheep. Considering demand-supply gap of the meat industry, and low replacement rate of indigenous caprine species, the conservative BMPR-1B locus can be explored, and FecB mutated goats can be produced. The experiment one produced CRISPR/Cas mediated KO transferable caprine embryos, and experiment two generated caprine embryos with desired FecB mutation using Easi-CRISPR strategy. In the KO experiment, Cas9 and BMPR-1B guide RNA (100:100ng/ul) were electroporated into single stage caprine zygotes at 750V, 10 ms and 1pulse using Neon transfection system. In the second experiment, phosphorothioate (PS) modified single-stranded oligodeoxynucleotide (ssODN) was used as an HDR template along with CRISPR components (100:100ng/ul, ssODN 100ng/ul). The precise time and method of electroporation, RNP format of CRISPR components and PS modified asymmetric ssODN were the factors that affected the production of mosaicism free BMPR-1B edited caprine embryos. The editing efficiency of KO and KI experiments was 68.52 and 63.16% respectively, and successful production of goats with higher mean ovulation rate can be realized with addition of embryo transfer technology to these experiments.
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Affiliation(s)
- Bosco Jose
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Meeti Punetha
- Division of Animal Physiology and Reproduction, ICAR-Central Institute for Research on Buffaloes, Hisar, Haryana, 125001, India.
| | - Manoj Kumar Tripathi
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Shivani Khanna
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Vijay Yadav
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Amit Kumar Singh
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Brijesh Kumar
- Division of Animal Reproduction, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Kiranjeet Singh
- Division of Surgery, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Vikrant Singh Chouhan
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India
| | - Mihir Sarkar
- Physiology & Climatology Division, ICAR-Indian Veterinary Research Institute (IVRI), Izatnagar, Bareilly, Uttar Pradesh, 243122, India.
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Nix JL, Schettini GP, Speckhart SL, Ealy AD, Biase FH. Ablation of OCT4 function in cattle embryos by double electroporation of CRISPR-Cas for DNA and RNA targeting (CRISPR-DART). PNAS NEXUS 2023; 2:pgad343. [PMID: 37954164 PMCID: PMC10637268 DOI: 10.1093/pnasnexus/pgad343] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 07/18/2023] [Accepted: 10/11/2023] [Indexed: 11/14/2023]
Abstract
CRISPR-Cas ribonucleoproteins (RNPs) are important tools for gene editing in preimplantation embryos. However, the inefficient production of biallelic deletions in cattle zygotes has hindered mechanistic studies of gene function. In addition, the presence of maternal RNAs that support embryo development until embryonic genome activation may cause confounding phenotypes. Here, we aimed to improve the efficiency of biallelic deletions and deplete specific maternal RNAs in cattle zygotes using CRISPR-Cas editing technology. Two electroporation sessions with Cas9D10A RNPs targeting exon 1 and the promoter of OCT4 produced biallelic deletions in 91% of the embryos tested. In most cases, the deletions were longer than 1,000 nucleotides long. Electroporation of Cas13a RNPs prevents the production of the corresponding proteins. We electroporated Cas9D10A RNPs targeting exon 1, including the promoter region, of OCT4 in two sessions with inclusion of Cas13a RNPs targeting OCT4 mRNAs in the second session to ablate OCT4 function in cattle embryos. A lack of OCT4 resulted in embryos arresting development prior to blastocyst formation at a greater proportion (13%) than controls (31.6%, P < 0.001). The few embryos that developed past the morula stage did not form a normal inner cell mass. Transcriptome analysis of single blastocysts, confirmed to lack exon 1 and promoter region of OCT4, revealed a significant (False Discovery Rate, FDR < 0.1) reduction in transcript abundance of many genes functionally connected to stemness, including markers of pluripotency (CADHD1, DPPA4, GNL3, RRM2). The results confirm that OCT4 is a key regulator of genes that modulate pluripotency and is required to form a functional blastocyst in cattle.
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Affiliation(s)
- Jada L Nix
- School of Animal Sciences, Virginia Polytechnic Institute and State University, 175 W Campus dr, Blacksburg, VA 24061, USA
| | - Gustavo P Schettini
- School of Animal Sciences, Virginia Polytechnic Institute and State University, 175 W Campus dr, Blacksburg, VA 24061, USA
| | - Savannah L Speckhart
- School of Animal Sciences, Virginia Polytechnic Institute and State University, 175 W Campus dr, Blacksburg, VA 24061, USA
| | - Alan D Ealy
- School of Animal Sciences, Virginia Polytechnic Institute and State University, 175 W Campus dr, Blacksburg, VA 24061, USA
| | - Fernando H Biase
- School of Animal Sciences, Virginia Polytechnic Institute and State University, 175 W Campus dr, Blacksburg, VA 24061, USA
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10
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Popova J, Bets V, Kozhevnikova E. Perspectives in Genome-Editing Techniques for Livestock. Animals (Basel) 2023; 13:2580. [PMID: 37627370 PMCID: PMC10452040 DOI: 10.3390/ani13162580] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/07/2023] [Revised: 08/08/2023] [Accepted: 08/08/2023] [Indexed: 08/27/2023] Open
Abstract
Genome editing of farm animals has undeniable practical applications. It helps to improve production traits, enhances the economic value of livestock, and increases disease resistance. Gene-modified animals are also used for biomedical research and drug production and demonstrate the potential to be used as xenograft donors for humans. The recent discovery of site-specific nucleases that allow precision genome editing of a single-cell embryo (or embryonic stem cells) and the development of new embryological delivery manipulations have revolutionized the transgenesis field. These relatively new approaches have already proven to be efficient and reliable for genome engineering and have wide potential for use in agriculture. A number of advanced methodologies have been tested in laboratory models and might be considered for application in livestock animals. At the same time, these methods must meet the requirements of safety, efficiency and availability of their application for a wide range of farm animals. This review aims at covering a brief history of livestock animal genome engineering and outlines possible future directions to design optimal and cost-effective tools for transgenesis in farm species.
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Affiliation(s)
- Julia Popova
- Laboratory of Bioengineering, Novosibirsk State Agrarian University, 630039 Novosibirsk, Russia; (J.P.); (V.B.)
| | - Victoria Bets
- Laboratory of Bioengineering, Novosibirsk State Agrarian University, 630039 Novosibirsk, Russia; (J.P.); (V.B.)
- Center of Technological Excellence, Novosibirsk State Technical University, 630073 Novosibirsk, Russia
| | - Elena Kozhevnikova
- Laboratory of Bioengineering, Novosibirsk State Agrarian University, 630039 Novosibirsk, Russia; (J.P.); (V.B.)
- Laboratory of Experimental Models of Cognitive and Emotional Disorders, Scientific-Research Institute of Neurosciences and Medicine, 630117 Novosibirsk, Russia
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11
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Giassetti MI, Miao D, Law NC, Oatley MJ, Park J, Robinson LD, Maddison LA, Bernhardt ML, Oatley JM. ARRDC5 expression is conserved in mammalian testes and required for normal sperm morphogenesis. Nat Commun 2023; 14:2111. [PMID: 37069147 PMCID: PMC10110545 DOI: 10.1038/s41467-023-37735-y] [Citation(s) in RCA: 3] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/25/2022] [Accepted: 03/28/2023] [Indexed: 04/19/2023] Open
Abstract
In sexual reproduction, sperm contribute half the genomic material required for creation of offspring yet core molecular mechanisms essential for their formation are undefined. Here, the α-arrestin molecule arrestin-domain containing 5 (ARRDC5) is identified as an essential regulator of mammalian spermatogenesis. Multispecies testicular tissue transcriptome profiling indicates that expression of Arrdc5 is testis enriched, if not specific, in mice, pigs, cattle, and humans. Knockout of Arrdc5 in mice leads to male specific sterility due to production of low numbers of sperm that are immotile and malformed. Spermiogenesis, the final phase of spermatogenesis when round spermatids transform to spermatozoa, is defective in testes of Arrdc5 deficient mice. Also, epididymal sperm in Arrdc5 knockouts are unable to capacitate and fertilize oocytes. These findings establish ARRDC5 as an essential regulator of mammalian spermatogenesis. Considering the role of arrestin molecules as modulators of cellular signaling and ubiquitination, ARRDC5 is a potential male contraceptive target.
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Affiliation(s)
- Mariana I Giassetti
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA
| | - Deqiang Miao
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA
| | - Nathan C Law
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- Department of Animal Sciences, Washington State University, Pullman, WA, USA
| | - Melissa J Oatley
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA
| | - Julie Park
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA
| | - LeeLa D Robinson
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA
| | - Lisette A Maddison
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
| | - Miranda L Bernhardt
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA
| | - Jon M Oatley
- Center for Reproductive Biology, Washington State University, Pullman, WA, USA.
- School of Molecular Biosciences, College of Veterinary Medicine, Washington State University, Pullman, WA, USA.
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12
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Wani AK, Akhtar N, Singh R, Prakash A, Raza SHA, Cavalu S, Chopra C, Madkour M, Elolimy A, Hashem NM. Genome centric engineering using ZFNs, TALENs and CRISPR-Cas9 systems for trait improvement and disease control in Animals. Vet Res Commun 2023; 47:1-16. [PMID: 35781172 DOI: 10.1007/s11259-022-09967-8] [Citation(s) in RCA: 7] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/26/2022] [Accepted: 06/24/2022] [Indexed: 01/27/2023]
Abstract
Livestock is an essential life commodity in modern agriculture involving breeding and maintenance. The farming practices have evolved mainly over the last century for commercial outputs, animal welfare, environment friendliness, and public health. Modifying genetic makeup of livestock has been proposed as an effective tool to create farmed animals with characteristics meeting modern farming system goals. The first technique used to produce transgenic farmed animals resulted in random transgene insertion and a low gene transfection rate. Therefore, genome manipulation technologies have been developed to enable efficient gene targeting with a higher accuracy and gene stability. Genome editing (GE) with engineered nucleases-Zinc finger nucleases (ZFNs) and transcription activator-like effector nucleases (TALENs) regulates the targeted genetic alterations to facilitate multiple genomic modifications through protein-DNA binding. The application of genome editors indicates usefulness in reproduction, animal models, transgenic animals, and cell lines. Recently, CRISPR/Cas system, an RNA-dependent genome editing tool (GET), is considered one of the most advanced and precise GE techniques for on-target modifications in the mammalian genome by mediating knock-in (KI) and knock-out (KO) of several genes. Lately, CRISPR/Cas9 tool has become the method of choice for genome alterations in livestock species due to its efficiency and specificity. The aim of this review is to discuss the evolution of engineered nucleases and GETs as a powerful tool for genome manipulation with special emphasis on its applications in improving economic traits and conferring resistance to infectious diseases of animals used for food production, by highlighting the recent trends for maintaining sustainable livestock production.
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Affiliation(s)
- Atif Khurshid Wani
- School of Bioengineering and Biosciences, Lovely Professional University, Punjab, 144411, India
| | - Nahid Akhtar
- School of Bioengineering and Biosciences, Lovely Professional University, Punjab, 144411, India
| | - Reena Singh
- School of Bioengineering and Biosciences, Lovely Professional University, Punjab, 144411, India
| | - Ajit Prakash
- Department of Biochemistry and Biophysics, University of North Carolina, 120 Mason Farm Road, CB# 7260, 3093 Genetic Medicine, Chapel Hill, NC, 27599-2760, USA
| | - Sayed Haidar Abbas Raza
- College of Animal Science and Technology, Northwest A&F University, Yangling, Shaanxi, China
| | - Simona Cavalu
- Faculty of Medicine and Pharmacy, University of Oradea, P -ta 1Decembrie 10, 410073, Oradea, Romania
| | - Chirag Chopra
- School of Bioengineering and Biosciences, Lovely Professional University, Punjab, 144411, India
| | - Mahmoud Madkour
- Animal Production Department, National Research Centre, Dokki, Giza, 12622, Egypt
| | - Ahmed Elolimy
- Animal Production Department, National Research Centre, Dokki, Giza, 12622, Egypt
| | - Nesrein M Hashem
- Department of Animal and Fish Production, Faculty of Agriculture (El-Shatby), Alexandria University, Alexandria, 21545, Egypt.
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13
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Li C, Du Y, Zhang T, Wang H, Hou Z, Zhang Y, Cui W, Chen W. "Genetic scissors" CRISPR/Cas9 genome editing cutting-edge biocarrier technology for bone and cartilage repair. Bioact Mater 2022; 22:254-273. [PMID: 36263098 PMCID: PMC9554751 DOI: 10.1016/j.bioactmat.2022.09.026] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/22/2022] [Revised: 09/13/2022] [Accepted: 09/28/2022] [Indexed: 12/02/2022] Open
Abstract
CRISPR/Cas9 is a revolutionary genome editing technology with the tremendous advantages such as precisely targeting/shearing ability, low cost and convenient operation, becoming an efficient and indispensable tool in biological research. As a disruptive technique, CRISPR/Cas9 genome editing has a great potential to realize a future breakthrough in the clinical bone and cartilage repairing as well. This review highlights the research status of CRISPR/Cas9 system in bone and cartilage repair, illustrates its mechanism for promoting osteogenesis and chondrogenesis, and explores the development tendency of CRISPR/Cas9 in bone and cartilage repair to overcome the current limitations.
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Affiliation(s)
- Chao Li
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China,Department of Orthopaedics, Shanghai Key Laboratory for Prevention and Treatment of Bone and Joint Diseases, Shanghai Institute of Traumatology and Orthopaedics, Ruijin Hospital, Shanghai Jiao Tong University School of Medicine, 197 Ruijin 2nd Road, Shanghai, 200025, PR China
| | - Yawei Du
- Department of Orthopaedics, Shanghai Key Laboratory for Prevention and Treatment of Bone and Joint Diseases, Shanghai Institute of Traumatology and Orthopaedics, Ruijin Hospital, Shanghai Jiao Tong University School of Medicine, 197 Ruijin 2nd Road, Shanghai, 200025, PR China
| | - Tongtong Zhang
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China
| | - Haoran Wang
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China,Department of Orthopaedics, Shanghai Key Laboratory for Prevention and Treatment of Bone and Joint Diseases, Shanghai Institute of Traumatology and Orthopaedics, Ruijin Hospital, Shanghai Jiao Tong University School of Medicine, 197 Ruijin 2nd Road, Shanghai, 200025, PR China
| | - Zhiyong Hou
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China
| | - Yingze Zhang
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China
| | - Wenguo Cui
- Department of Orthopaedics, Shanghai Key Laboratory for Prevention and Treatment of Bone and Joint Diseases, Shanghai Institute of Traumatology and Orthopaedics, Ruijin Hospital, Shanghai Jiao Tong University School of Medicine, 197 Ruijin 2nd Road, Shanghai, 200025, PR China,Corresponding author.
| | - Wei Chen
- Department of Orthopaedics, The Third Hospital of Hebei Medical University, Orthopaedic Research Institution of Hebei Province, NHC Key Laboratory of Intelligent Orthopaedic Equipment, No.139 Ziqiang Road, Shijiazhuang, 050051, PR China,Corresponding author.
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14
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Miskel D, Poirier M, Beunink L, Rings F, Held E, Tholen E, Tesfaye D, Schellander K, Salilew-Wondim D, Blaschka C, Große-Brinkhaus C, Brenig B, Hoelker M. The cell cycle stage of bovine zygotes electroporated with CRISPR/Cas9-RNP affects frequency of Loss-of-heterozygosity editing events. Sci Rep 2022; 12:10793. [PMID: 35750764 PMCID: PMC9232522 DOI: 10.1038/s41598-022-14699-5] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/14/2021] [Accepted: 06/10/2022] [Indexed: 12/14/2022] Open
Abstract
At the embryonic level, CRISPR technologies have been used to edit genomes reliably and efficiently in various mammalian models, with Ribonucleoprotein (RNP) electroporation potentially representing a superior delivery method into mammalian zygotes. However, detailed insights of the interactions between varying technical settings as well as the time point of electroporation in a bovine zygote's cell cycle on developmental metrics and the frequency and type of editing events are largely unknown. The present study uncovers that increasing pulse lengths result in higher Full Edit rates, with Mosaicism in Full-Edit embryos being significantly affected by adjusting RNP-electroporation relative to zygote cell cycle. A considerable proportion of Full Edit embryos demonstrated loss-of-heterozygosity after RNP-electroporation prior to S-phase. Some of these loss-of-heterozygosity events are a consequence of chromosomal disruptions along large sections of the target chromosomes making it necessary to check for their presence prior use of this technique in animal breeding. One out of 2 of these loss-of-heterozygosity events, however, was not associated with loss of an entire chromosome or chromosomal sections. Whether analysed loss-of-heterozygosity in these cases, however, was a false negative result due to loss of PCR primer sequences after INDEL formation at the target side or indeed due to interhomolog recombination needs to be clarified in follow up studies since the latter would for sure offer attractive options for future breeding schedules.
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Affiliation(s)
- Dennis Miskel
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Mikhael Poirier
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Luisa Beunink
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Franca Rings
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Eva Held
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Ernst Tholen
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Dawit Tesfaye
- grid.47894.360000 0004 1936 8083Department of Biomedical Sciences, Animal Reproduction and Biotechnology Laboratory, Colorado State University, 3105 Rampart Rd, Fort Collins, CO 80521 USA
| | - Karl Schellander
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Dessie Salilew-Wondim
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Carina Blaschka
- grid.7450.60000 0001 2364 4210Department of Animal Science, Biotechnology and Reproduction of Farm Animals, Georg August University Goettingen, Burckhardtweg 2, 37077 Goettingen, Germany
| | - Christine Große-Brinkhaus
- grid.10388.320000 0001 2240 3300Institute of Animal Sciences, Animal Breeding, University of Bonn, Endenicher Allee 15, 53115 Bonn, Germany
| | - Bertram Brenig
- grid.7450.60000 0001 2364 4210Department of Molecular Biology of Livestock, Institute of Veterinary Medicine, Georg August University Goettingen, Burckhardtweg 2, 37077 Goettingen, Germany
| | - Michael Hoelker
- grid.7450.60000 0001 2364 4210Department of Animal Science, Biotechnology and Reproduction of Farm Animals, Georg August University Goettingen, Burckhardtweg 2, 37077 Goettingen, Germany
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15
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Gewiss RL, Law NC, Helsel AR, Shelden EA, Griswold MD. Two distinct Sertoli cell states are regulated via germ cell crosstalk. Biol Reprod 2021; 105:1591-1602. [PMID: 34494084 PMCID: PMC8689118 DOI: 10.1093/biolre/ioab160] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/05/2021] [Revised: 07/30/2021] [Accepted: 08/13/2021] [Indexed: 01/15/2023] Open
Abstract
Sertoli cells are a critical component of the testis environment for their role in maintaining seminiferous tubule structure, establishing the blood-testis barrier, and nourishing maturing germ cells in a specialized niche. This study sought to uncover how Sertoli cells are regulated in the testis environment via germ cell crosstalk in the mouse. We found two major clusters of Sertoli cells as defined by their transcriptomes in Stages VII-VIII of the seminiferous epithelium and a cluster for all other stages. Additionally, we examined transcriptomes of germ cell-deficient testes and found that these existed in a state independent of either of the germ cell-sufficient clusters. Together, we highlight two main transcriptional states of Sertoli cells in an unperturbed testis environment, and a germ cell-deficient environment does not allow normal Sertoli cell transcriptome cycling and results in a state unique from either of those seen in Sertoli cells from a germ cell-sufficient environment.
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Affiliation(s)
- Rachel L Gewiss
- School of Molecular Biosciences, Washington State University, Pullman, Washington, USA.,Center for Reproductive Biology, Washington State University, Pullman, Washington, USA
| | - Nathan C Law
- Center for Reproductive Biology, Washington State University, Pullman, Washington, USA.,Department of Animal Sciences, Washington State University, Pullman, Washington, USA
| | - Aileen R Helsel
- School of Molecular Biosciences, Washington State University, Pullman, Washington, USA.,Center for Reproductive Biology, Washington State University, Pullman, Washington, USA
| | - Eric A Shelden
- School of Molecular Biosciences, Washington State University, Pullman, Washington, USA.,Center for Reproductive Biology, Washington State University, Pullman, Washington, USA
| | - Michael D Griswold
- School of Molecular Biosciences, Washington State University, Pullman, Washington, USA.,Center for Reproductive Biology, Washington State University, Pullman, Washington, USA
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16
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Lin JC, Van Eenennaam AL. Electroporation-Mediated Genome Editing of Livestock Zygotes. Front Genet 2021; 12:648482. [PMID: 33927751 PMCID: PMC8078910 DOI: 10.3389/fgene.2021.648482] [Citation(s) in RCA: 12] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/31/2020] [Accepted: 03/22/2021] [Indexed: 12/20/2022] Open
Abstract
The introduction of genome editing reagents into mammalian zygotes has traditionally been accomplished by cytoplasmic or pronuclear microinjection. This time-consuming procedure requires expensive equipment and a high level of skill. Electroporation of zygotes offers a simplified and more streamlined approach to transfect mammalian zygotes. There are a number of studies examining the parameters used in electroporation of mouse and rat zygotes. Here, we review the electroporation conditions, timing, and success rates that have been reported for mice and rats, in addition to the few reports about livestock zygotes, specifically pigs and cattle. The introduction of editing reagents at, or soon after, fertilization can help reduce the rate of mosaicism, the presence of two of more genotypes in the cells of an individual; as can the introduction of nuclease proteins rather than mRNA encoding nucleases. Mosaicism is particularly problematic in large livestock species with long generation intervals as it can take years to obtain non-mosaic, homozygous offspring through breeding. Gene knockouts accomplished via the non-homologous end joining pathway have been more widely reported and successfully accomplished using electroporation than have gene knock-ins. Delivering large DNA plasmids into the zygote is hindered by the zona pellucida (ZP), and the majority of gene knock-ins accomplished by electroporation have been using short single stranded DNA (ssDNA) repair templates, typically less than 1 kb. The most promising approach to deliver larger donor repair templates of up to 4.9 kb along with genome editing reagents into zygotes, without using cytoplasmic injection, is to use recombinant adeno-associated viruses (rAAVs) in combination with electroporation. However, similar to other methods used to deliver clustered regularly interspaced palindromic repeat (CRISPR) genome-editing reagents, this approach is also associated with high levels of mosaicism. Recent developments complementing germline ablated individuals with edited germline-competent cells offer an approach to avoid mosaicism in the germline of genome edited founder lines. Even with electroporation-mediated delivery of genome editing reagents to mammalian zygotes, there remain additional chokepoints in the genome editing pipeline that currently hinder the scalable production of non-mosaic genome edited livestock.
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Affiliation(s)
- Jason C Lin
- Department of Animal Science, University of California, Davis, Davis, CA, United States
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17
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Tanihara F, Hirata M, Nguyen NT, Le QA, Wittayarat M, Fahrudin M, Hirano T, Otoi T. Generation of CD163-edited pig via electroporation of the CRISPR/Cas9 system into porcine in vitro-fertilized zygotes. Anim Biotechnol 2021; 32:147-154. [PMID: 31558095 DOI: 10.1080/10495398.2019.1668801] [Citation(s) in RCA: 11] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/20/2022]
Abstract
CD163 is a putative fusion receptor for virus of porcine reproductive and respiratory syndrome (PRRS). In this study, we introduced a CRISPR/Cas9 system [guide RNAs (gRNAs) with Cas9 protein] targeting the CD163 gene into in vitro-fertilized porcine zygotes by electroporation to generate CD163-modified pigs. First, we designed four types of gRNAs that targeted distinct sites in exon 7 of the CD163 gene. Cas9 protein with different gRNAs was introduced into in vitro-fertilized zygotes by electroporation. When the electroporated zygotes were allowed to develop to blastocysts in vitro and the genome editing efficiency was evaluated using these blastocysts, three (gRNA1, 2, and 4) of the four gRNAs tested successfully edited the CD163 gene. To generate CD163-knockout pigs, a total of 200 electroporated zygotes using these three gRNAs were transferred into the oviducts of oestrous-synchronized surrogate and the surrogate gave birth to eight piglets. Subsequent sequence analysis revealed that one of the piglets carried no wild-type sequence in CD163 gene. The other seven piglets carried only wild-type sequence. Thus, we successfully generated a CD163-edited pig by electroporation of the CRISPR/Cas9 system into in vitro-fertilized zygotes, although further improvement is required to generate genetically modified pigs with high efficiency.
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Affiliation(s)
- Fuminori Tanihara
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
| | - Maki Hirata
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
| | - Nhien Thi Nguyen
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
| | - Quynh Anh Le
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
| | - Manita Wittayarat
- Faculty of Veterinary Science, Prince of Songkla University, Songkhla, Thailand
| | - Mokhamad Fahrudin
- Faculty of Veterinary Science, Bogor Agricultural University, Bogor, Indonesia
| | - Takayuki Hirano
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
| | - Takeshige Otoi
- Laboratory of Animal Reproduction, Faculty of Bioscience and Bioindustry, Tokushima University, Tokushima, Japan
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18
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Campanile G, Baruselli PS, Limone A, D'Occhio MJ. Local action of cytokines and immune cells in communication between the conceptus and uterus during the critical period of early embryo development, attachment and implantation - Implications for embryo survival in cattle: A review. Theriogenology 2021; 167:1-12. [PMID: 33743503 DOI: 10.1016/j.theriogenology.2021.02.020] [Citation(s) in RCA: 11] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/19/2020] [Revised: 02/15/2021] [Accepted: 02/24/2021] [Indexed: 12/16/2022]
Abstract
Early embryo development, implantation and pregnancy involve a complex dialogue between the embryo and mother. In cattle this dialogue starts as early as days 3-4 when the embryo is still in the oviduct, and it continues to implantation. Immunological processes involving cytokines, mast cells and macrophages form an important part of this dialogue. Amongst the cytokines, interleukin-6 (Il-6) and leukemia inhibitory factor (LIF) are secreted by both the embryo and uterine endometrium and form part of an ongoing and reciprocating dialogue. Mast cells and macrophages populate the uterine endometrium during embryo development and are involved in achieving the correct balance between inflammatory and anti-inflammatory reactions at the uterus that are associated with embryo attachment and implantation. Embryo loss is the major cause of reproductive wastage in cattle, and livestock generally. A deeper understanding of immunological processes during early embryo development will help to achieve the next step change in the efficiency of natural and assisted breeding.
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Affiliation(s)
- Giuseppe Campanile
- Department of Veterinary Medicine and Animal Production, University of Naples Federico II, Naples, Italy.
| | - Pietro S Baruselli
- Department of Animal Reproduction, Faculty of Veterinary Medicine and Animal Science, University of Sao Paulo, Sao Paulo, Brazil.
| | - Antonio Limone
- Instituto Zooprofilattico Sperimentale Del Mezzogiorno, Portici, Naples, Italy
| | - Michael J D'Occhio
- School of Life and Environmental Sciences, Faculty of Science, The University of Sydney, New South Wales, 2006, Australia
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19
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Perisse IV, Fan Z, Singina GN, White KL, Polejaeva IA. Improvements in Gene Editing Technology Boost Its Applications in Livestock. Front Genet 2021; 11:614688. [PMID: 33603767 PMCID: PMC7885404 DOI: 10.3389/fgene.2020.614688] [Citation(s) in RCA: 21] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/06/2020] [Accepted: 12/07/2020] [Indexed: 12/18/2022] Open
Abstract
Accelerated development of novel CRISPR/Cas9-based genome editing techniques provides a feasible approach to introduce a variety of precise modifications in the mammalian genome, including introduction of multiple edits simultaneously, efficient insertion of long DNA sequences into specific targeted loci as well as performing nucleotide transitions and transversions. Thus, the CRISPR/Cas9 tool has become the method of choice for introducing genome alterations in livestock species. The list of new CRISPR/Cas9-based genome editing tools is constantly expanding. Here, we discuss the methods developed to improve efficiency and specificity of gene editing tools as well as approaches that can be employed for gene regulation, base editing, and epigenetic modifications. Additionally, advantages and disadvantages of two primary methods used for the production of gene-edited farm animals: somatic cell nuclear transfer (SCNT or cloning) and zygote manipulations will be discussed. Furthermore, we will review agricultural and biomedical applications of gene editing technology.
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Affiliation(s)
- Iuri Viotti Perisse
- Department of Animal, Dairy and Veterinary Sciences, Utah State University, Logan, UT, United States
| | - Zhiqiang Fan
- Department of Animal, Dairy and Veterinary Sciences, Utah State University, Logan, UT, United States
| | - Galina N. Singina
- L.K. Ernst Federal Research Center for Animal Husbandry, Podolsk, Russia
| | - Kenneth L. White
- Department of Animal, Dairy and Veterinary Sciences, Utah State University, Logan, UT, United States
| | - Irina A. Polejaeva
- Department of Animal, Dairy and Veterinary Sciences, Utah State University, Logan, UT, United States
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20
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Owen JR, Hennig SL, McNabb BR, Lin JC, Young AE, Murray JD, Ross PJ, Van Eenennaam AL. Harnessing endogenous repair mechanisms for targeted gene knock-in of bovine embryos. Sci Rep 2020; 10:16031. [PMID: 32994506 PMCID: PMC7525238 DOI: 10.1038/s41598-020-72902-x] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/09/2020] [Accepted: 09/04/2020] [Indexed: 01/06/2023] Open
Abstract
Introducing useful traits into livestock breeding programs through gene knock-ins has proven challenging. Typically, targeted insertions have been performed in cell lines, followed by somatic cell nuclear transfer cloning, which can be inefficient. An alternative is to introduce genome editing reagents and a homologous recombination (HR) donor template into embryos to trigger homology directed repair (HDR). However, the HR pathway is primarily restricted to actively dividing cells (S/G2-phase) and its efficiency for the introduction of large DNA sequences in zygotes is low. The homology-mediated end joining (HMEJ) approach has been shown to improve knock-in efficiency in non-dividing cells and to harness HDR after direct injection of embryos. The knock-in efficiency for a 1.8 kb gene was contrasted when combining microinjection of a gRNA/Cas9 ribonucleoprotein complex with a traditional HR donor template or an HMEJ template in bovine zygotes. The HMEJ template resulted in a significantly higher rate of gene knock-in as compared to the HR template (37.0% and 13.8%; P < 0.05). Additionally, more than a third of the knock-in embryos (36.9%) were non-mosaic. This approach will facilitate the one-step introduction of gene constructs at a specific location of the bovine genome and contribute to the next generation of elite cattle.
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Affiliation(s)
- Joseph R Owen
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
| | - Sadie L Hennig
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
| | - Bret R McNabb
- Department of Population Health and Reproduction, School of Veterinary Medicine, University of CA - Davis, Davis, CA, USA
| | - Jason C Lin
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
| | - Amy E Young
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
| | - James D Murray
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
- Department of Population Health and Reproduction, School of Veterinary Medicine, University of CA - Davis, Davis, CA, USA
| | - Pablo J Ross
- Department of Animal Science, University of CA - Davis, Davis, CA, USA
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21
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Donor-derived spermatogenesis following stem cell transplantation in sterile NANOS2 knockout males. Proc Natl Acad Sci U S A 2020; 117:24195-24204. [PMID: 32929012 PMCID: PMC7533891 DOI: 10.1073/pnas.2010102117] [Citation(s) in RCA: 38] [Impact Index Per Article: 9.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/02/2023] Open
Abstract
Spermatogonial stem cell transplantation (SSCT) is an experimental technique for transfer of germline between donor and recipient males that could be used as a tool for biomedical research, preservation of endangered species, and dissemination of desirable genetics in food animal populations. To fully realize these potentials, recipient males must be devoid of endogenous germline but possess normal testicular architecture and somatic cell function capable of supporting allogeneic donor stem cell engraftment and regeneration of spermatogenesis. Here we show that male mice, pigs, goats, and cattle harboring knockout alleles of the NANOS2 gene generated by CRISPR-Cas9 editing have testes that are germline ablated but otherwise structurally normal. In adult pigs and goats, SSCT with allogeneic donor stem cells led to sustained donor-derived spermatogenesis. With prepubertal mice, allogeneic SSCT resulted in attainment of natural fertility. Collectively, these advancements represent a major step toward realizing the enormous potential of surrogate sires as a tool for dissemination and regeneration of germplasm in all mammalian species.
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Camargo LSA, Owen JR, Van Eenennaam AL, Ross PJ. Efficient One-Step Knockout by Electroporation of Ribonucleoproteins Into Zona-Intact Bovine Embryos. Front Genet 2020; 11:570069. [PMID: 33133156 PMCID: PMC7504904 DOI: 10.3389/fgene.2020.570069] [Citation(s) in RCA: 12] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/06/2020] [Accepted: 08/12/2020] [Indexed: 12/16/2022] Open
Abstract
Somatic cell nuclear transfer or cytoplasm microinjection have been used to generate genome-edited farm animals; however, these methods have several drawbacks that reduce their efficiency. This study aimed to develop electroporation conditions that allow delivery of CRISPR/Cas9 system to bovine zygotes for efficient gene knock-out. We optimized electroporation conditions to deliver Cas9:sgRNA ribonucleoproteins to bovine zygotes without compromising embryo development. Higher electroporation pulse voltage resulted in increased membrane permeability; however, voltages above 15 V/mm decreased embryo developmental potential. The zona pellucida of bovine embryos was not a barrier to efficient RNP electroporation. Using parameters optimized for maximal membrane permeability while maintaining developmental competence we achieved high rates of gene editing when targeting bovine OCT4, which resulted in absence of OCT4 protein in 100% of the evaluated embryos and the expected arrest of embryonic development at the morula stage. In conclusion, Cas9:sgRNA ribonucleoproteins can be delivered efficiently by electroporation to zona-intact bovine zygotes, resulting in efficient gene knockouts.
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Affiliation(s)
| | - Joseph R Owen
- Department of Animal Science, University of California, Davis, Davis, CA, United States
| | | | - Pablo Juan Ross
- Department of Animal Science, University of California, Davis, Davis, CA, United States
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23
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Menchaca A, Dos Santos-Neto PC, Mulet AP, Crispo M. CRISPR in livestock: From editing to printing. Theriogenology 2020; 150:247-254. [PMID: 32088034 PMCID: PMC7102594 DOI: 10.1016/j.theriogenology.2020.01.063] [Citation(s) in RCA: 32] [Impact Index Per Article: 8.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/22/2020] [Accepted: 01/28/2020] [Indexed: 12/16/2022]
Abstract
Precise genome editing of large animals applied to livestock and biomedicine is nowadays possible since the CRISPR revolution. This review summarizes the latest advances and the main technical issues that determine the success of this technology. The pathway from editing to printing, from engineering the genome to achieving the desired animals, does not always imply an easy, fast and safe journey. When applied in large animals, CRISPR involves time- and cost-consuming projects, and it is mandatory not only to choose the best approach for genome editing, but also for embryo production, zygote microinjection or electroporation, cryopreservation and embryo transfer. The main technical refinements and most frequent questions to improve this disruptive biotechnology in large animals are presented. In addition, we discuss some CRISPR applications to enhance livestock production in the context of a growing global demand of food, in terms of increasing efficiency, reducing the impact of farming on the environment, enhancing pest control, animal welfare and health. The challenge is no longer technical. Controversies and consensus, opportunities and threats, benefits and risks, ethics and science should be reconsidered to enter into the CRISPR era.
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Affiliation(s)
- A Menchaca
- Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Cruz del Sur 2350, Montevideo, Uruguay.
| | - P C Dos Santos-Neto
- Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Cruz del Sur 2350, Montevideo, Uruguay
| | - A P Mulet
- Unidad de Animales Transgénicos y de Experimentación (UATE), Institut Pasteur de Montevideo, Mataojo, 2020, Montevideo, Uruguay
| | - M Crispo
- Unidad de Animales Transgénicos y de Experimentación (UATE), Institut Pasteur de Montevideo, Mataojo, 2020, Montevideo, Uruguay
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Livestock Gene Editing by One-step Embryo Manipulation. J Equine Vet Sci 2020; 89:103025. [PMID: 32563448 DOI: 10.1016/j.jevs.2020.103025] [Citation(s) in RCA: 19] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/18/2020] [Revised: 04/06/2020] [Accepted: 04/07/2020] [Indexed: 12/11/2022]
Abstract
The breakthrough and rapid advance of clustered regularly interspaced short palindromic repeat (CRISPR)/CRISPR-associated protein 9 (Cas9) technology has enabled the efficient generation of gene-edited animals by one-step embryo manipulation. Clustered regularly interspaced short palindromic repeat/CRISPR-associated protein 9 delivery to the livestock embryos has been typically achieved by intracytoplasmic microinjection; however, recent studies show that electroporation may be a reliable, efficient, and practical method for CRISPR/Cas9 delivery. The source of embryos used to generate gene-edited animals varies from in vivo to in vitro produced, depending mostly on the species of interest. In addition, different Cas9 and gRNA reagents can be used for embryo editing, ranging from Cas9-coding plasmid or messenger RNA to Cas9 recombinant protein, which can be combined with in vitro transcribed or synthetic guide RNAs. Mosaicism is reported as one of the main problems with generation of animals by embryo editing. On the other hand, off-target mutations are rarely found in livestock derived from one-step editing. In this review, we discussed these and other aspects of generating gene-edited animals by single-step embryo manipulation.
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Blastocyst hatching site is regularly distributed and does not influence foetal development in mice. Sci Rep 2020; 10:2475. [PMID: 32051520 PMCID: PMC7015891 DOI: 10.1038/s41598-020-59424-2] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/30/2019] [Accepted: 01/27/2020] [Indexed: 11/08/2022] Open
Abstract
Hatching out from the zona pellucida (ZP) is a crucial step for blastocyst implantation and development. However, it is still unknown whether the location of the hatching site relative to the inner cell mass (ICM) affects embryo implantation and foetal development. Here, we classified hatching blastocysts into three categories, 0° ≤ θ ≤ 30°, 30° < θ ≤ 60°, and 60° < θ ≤ 90°, in which θ is determined based on the relative position of the hatching site to the arc midpoint of the ICM. Non-surgical embryo transfer (NSET) devices were employed to evaluate blastocyst implantation and embryo development. Of 1,827 hatching blastocysts, 43.84%, 30.60%, and 21.67% were categorized as 30° < θ ≤ 60°, 0° ≤ θ ≤ 30°, and 60° < θ ≤ 90°, respectively. Embryos with different hatching sites showed no distinct differences in blastocyst implantation; surrogate female pregnancy; embryo development to term; litter size, or offspring survival, gender, or body weight. Our results indicate that mouse blastocyst hatching site is not randomly distributed. Embryo implantation and development are not correlated with the blastocyst hatching site in mice. Thus, assessment of the blastocyst hatching site should not be recommended to evaluate mouse blastocyst implantation and developmental potential.
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Bishop TF, Van Eenennaam AL. Genome editing approaches to augment livestock breeding programs. ACTA ACUST UNITED AC 2020; 223:223/Suppl_1/jeb207159. [PMID: 32034040 DOI: 10.1242/jeb.207159] [Citation(s) in RCA: 28] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/18/2022]
Abstract
The prospect of genome editing offers a number of promising opportunities for livestock breeders. Firstly, these tools can be used in functional genomics to elucidate gene function, and identify causal variants underlying monogenic traits. Secondly, they can be used to precisely introduce useful genetic variation into structured livestock breeding programs. Such variation may include repair of genetic defects, the inactivation of undesired genes, and the moving of useful alleles and haplotypes between breeds in the absence of linkage drag. Editing could also be used to accelerate the rate of genetic progress by enabling the replacement of the germ cell lineage of commercial breeding animals with cells derived from genetically elite lines. In the future, editing may also provide a useful complement to evolving approaches to decrease the length of the generation interval through in vitro generation of gametes. For editing to be adopted, it will need to seamlessly integrate with livestock breeding schemes. This will likely involve introducing edits into multiple elite animals to avoid genetic bottlenecks. It will also require editing of different breeds and lines to maintain genetic diversity, and enable structured cross-breeding. This requirement is at odds with the process-based trigger and event-based regulatory approach that has been proposed for the products of genome editing by several countries. In the absence of regulatory harmony, researchers in some countries will have the ability to use genome editing in food animals, while others will not, resulting in disparate access to these tools, and ultimately the potential for global trade disruptions.
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McFarlane GR, Salvesen HA, Sternberg A, Lillico SG. On-Farm Livestock Genome Editing Using Cutting Edge Reproductive Technologies. FRONTIERS IN SUSTAINABLE FOOD SYSTEMS 2019. [DOI: 10.3389/fsufs.2019.00106] [Citation(s) in RCA: 18] [Impact Index Per Article: 3.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/24/2023] Open
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