Gene transfer by electroporation, lipofection, and DEAE-dextran transfection: compatibility with cell-sorting by flow cytometry

Generation of mutant pigs by lipofection-mediated genome editing in embryos

The specificity and efficiency of CRISPR/Cas9 gene-editing systems are determined by several factors, including the mode of delivery, when applied to mammalian embryos. Given the limited time window for delivery, faster and more reliable methods to introduce Cas9-gRNA ribonucleoprotein complexes (RNPs) into target embryos are needed. In pigs, somatic cell nuclear transfer using gene-modified somatic cells and the direct introduction of gene editors into the cytoplasm of zygotes/embryos by microinjection or electroporation have been used to generate gene-edited embryos; however, these strategies require expensive equipment and sophisticated techniques. In this study, we developed a novel lipofection-mediated RNP transfection technique that does not require specialized equipment for the generation of gene-edited pigs and produced no detectable off-target events. In particular, we determined the concentration of lipofection reagent for efficient RNP delivery into embryos and successfully generated MSTN gene-edited pigs (with mutations in 7 of 9 piglets) after blastocyst transfer to a recipient gilt. This newly established lipofection-based technique is still in its early stages and requires improvements, particularly in terms of editing efficiency. Nonetheless, this practical method for rapid and large-scale lipofection-mediated gene editing in pigs has important agricultural and biomedical applications.

Modification of the Genome of Domestic Animals

In the past few years, new technologies have arisen that enable higher efficiency of gene editing. With the increase ease of using gene editing technologies, it is important to consider the best method for transferring new genetic material to livestock animals. Microinjection is a technique that has proven to be effective in mice but is less efficient in large livestock animals. Over the years, a variety of methods have been used for cloning as well as gene transfer including; nuclear transfer, sperm mediated gene transfer (SMGT), and liposome-mediated DNA transfer. This review looks at the different success rate of these methods and how they have evolved to become more efficient. As well as gene editing technologies, including Zinc-finger nucleases (ZFNs), transcription activator-like effector nucleases (TALENs), and the most recent clustered regulatory interspaced short palindromic repeats (CRISPRs). Through the advancements in gene-editing technologies, generating transgenic animals is now more accessible and affordable. The goals of producing transgenic animals are to 1) increase our understanding of biology and biomedical science; 2) increase our ability to produce more efficient animals; and 3) produce disease resistant animals. ZFNs, TALENs, and CRISPRs combined with gene transfer methods increase the possibility of achieving these goals.

Transgenic animals in biomedicine and agriculture: outlook for the future

Transgenic animals are produced by introduction of 'foreign' deoxyribonucleic acid (DNA) into preimplantation embryos. The foreign DNA is inserted into the genetic material and may be expressed in tissues of the resulting individual. This technique is of great importance to many aspects of biomedical science including gene regulation, the immune system, cancer research, developmental biology, biomedicine, manufacturing and agriculture. The production of transgenic animals is one of a number of new and developing technologies that will have a profound impact on the genetic improvement of livestock. The rate at which these technologies are incorporated into production schemes will determine the speed at which we will be able to achieve our goal of more efficiently producing livestock, which meets consumer and market demand.

Targeted gene transfer to corneal stroma in vivo by electric pulses

This study was conducted to develop a method of targeted gene transfer by electric pulses to a selected area of corneal stroma in vivo. Plasmid DNA with a green fluorescent protein (GFP) gene under a cytomegalovirus promoter was injected through the corneal pocket into the corneal stroma of the adult Brown Norway rat, and various intensities of electric pulses ranging from 10 to 30 V were delivered to the corneal epithelial side with an electric probe. Direct stereomicroscopy of the fluorescent using real-time imaging was used to determine in vivo gene expression on days 1, 2, 4, 6, 8, 10, 15, and 20 after gene transfer. Transgene expression was detected in the corneal stroma as early as day 1 and until day 15. The most intense expression was noted on days 4 and 6. Gene transfer was most effective using eight electric pulses of 20 V for 50 msec. Histologic study disclosed GFP expression in keratocytes within the targeted area. There was no apparent cell damage in the gene transferred cells. No apparent inflammation was found in the anterior chamber or trabecular cells when electric pulses less than 30 V were used. In summary, the present technique transferred the gene of interest to a highly selected area of corneal stroma with no apparent damage. This method will likely be useful not only for developing gene therapy for corneal diseases but also for corneal research in general.