High-throughput library transgenesis in Caenorhabditis elegans via Transgenic Arrays Resulting in Diversity of Integrated Sequences (TARDIS).

High-throughput transgenesis using synthetic DNA libraries is a powerful method for systematically exploring genetic function. Diverse synthesized libraries have been used for protein engineering, identification of protein-protein interactions, characterization of promoter libraries, developmental and evolutionary lineage tracking, and various other exploratory assays. However, the need for library transgenesis has effectively restricted these approaches to single-cell models. Here, we present Transgenic Arrays Resulting in Diversity of Integrated Sequences (TARDIS), a simple yet powerful approach to large-scale transgenesis that overcomes typical limitations encountered in multicellular systems. TARDIS splits the transgenesis process into a two-step process: creation of individuals carrying experimentally introduced sequence libraries, followed by inducible extraction and integration of individual sequences/library components from the larger library cassette into engineered genomic sites. Thus, transformation of a single individual, followed by lineage expansion and functional transgenesis, gives rise to thousands of genetically unique transgenic individuals. We demonstrate the power of this system using engineered, split selectable TARDIS sites in Caenorhabditis elegans to generate (1) a large set of individually barcoded lineages and (2) transcriptional reporter lines from predefined promoter libraries. We find that this approach increases transformation yields up to approximately 1000-fold over current single-step methods. While we demonstrate the utility of TARDIS using C. elegans, in principle the process is adaptable to any system where experimentally generated genomic loci landing pads and diverse, heritable DNA elements can be generated.

Transgenesis ­ the ability to insert foreign genetic material (known as transgenes) in to the genome of an organism ­ has revolutionized biological research. This approach has made it possible for scientists to study the role of specific genes and to produce animal models which mimic aspects of human diseases. For transgenes to be maintained and passed down to future generations, they must be introduced into germ cells which will go on to form the egg and sperm of the organism. However, despite advances in genetic engineering, this process (called 'specific transgenesis') is still laborious and time-consuming, and limits researchers to working with only a small number of known DNA sequences at a time. In contrast, 'exploratory transgenesis' ­ where dozens of transgenes from a library of DNA sequences are introduced simultaneously into multiple individuals ­ is more efficient and allows for more large-scale experiments. However, this approach can only be done with single-celled organisms like bacteria, and remains virtually impossible in laboratory animals like worms or mice. Stevenson et al. therefore set out to boost the efficiency of exploratory transgenesis in a commonly used laboratory animal, the roundworm Caenorhabditis elegans. To do this, they used the 'library' principle of exploratory transgenesis in order to develop a new resource called TARDIS (short for, Transgenic Arrays Resulting in Diversity of Integrated Sequences). First, Stevenson et al. genetically engineered worms to carry a 'landing site' for foreign DNA. Next, a library of transgenes and a mechanism which cuts pieces of DNA and pastes them into the landing site were introduced into the germ cells of these worms using traditional methods. The worms were then bred to generate a large population of offspring that had inherited this array of foreign DNA sequences. Finally, the 'cut and paste' mechanism was switched on and a random transgene was inserted into the landing site in the genome. This resulted in thousands of worms which each had a unique genetic modification that can be passed on to future generations. These results show for the first time that larger-scale transgenesis experiments are possible in multi-cellular animals. In the future, Stevenson et al. hope that TARDIS can be adapted to different organisms and allow researchers to carry out experiments that were not previously possible.

Sexual Dimorphism through the Lens of Genome Manipulation, Forward Genetics, and Spatiotemporal Sequencing.

Sexual reproduction often leads to selection that favors the evolution of sex-limited traits or sex-specific variation for shared traits. These sexual dimorphisms manifest due to sex-specific genetic architectures and sex-biased gene expression across development, yet the molecular mechanisms underlying these patterns are largely unknown. The first step is to understand how sexual dimorphisms arise across the genotype-phenotype-fitness map. The emergence of "4D genome technologies" allows for efficient, high-throughput, and cost-effective manipulation and observations of this process. Studies of sexual dimorphism will benefit from combining these technological advances (e.g., precision genome editing, inducible transgenic systems, and single-cell RNA sequencing) with clever experiments inspired by classic designs (e.g., bulked segregant analysis, experimental evolution, and pedigree tracing). This perspective poses a synthetic view of how manipulative approaches coupled with cutting-edge observational methods and evolutionary theory are poised to uncover the molecular genetic basis of sexual dimorphism with unprecedented resolution. We outline hypothesis-driven experimental paradigms for identifying genetic mechanisms of sexual dimorphism among tissues, across development, and over evolutionary time.

Rapid Self-Selecting and Clone-Free Integration of Transgenes into Engineered CRISPR Safe Harbor Locations in Caenorhabditis elegans.

Precision genome editing for model organisms has revolutionized functional analysis and validation of a wide variety of molecular systems. To date, the capacity to insert single-copy transgenes into the model nematode Caenorhabditis elegans has focused on utilizing either transposable elements or CRISPR-based safe harbor strategies. These methods require plate-level screening processes to avoid selecting heritable extrachromosomal arrays or rely on co-CRISPR markers to identify knock-in events. As a result, verification of transgene insertion requires anti-array selection screening methods and PCR genotyping. These approaches also rely on cloning plasmids for the addition of transgenes. Here, we present a novel safe harbor CRISPR-based integration strategy that utilizes engineered insertion locations containing a synthetic guide RNA target and a split-selection system to eliminate false positives from array formation, thereby providing integration-specific selection. This approach allows the experimenter to confirm an integration event has taken place without molecular validation or anti-array screening methods and is capable of producing integrated transgenic lines in as little as five days post-injection. To further increase the speed of generating transgenic lines, we also utilized the C. elegans native microhomology-based recombination, to assemble transgenes in-situ, removing the cloning step. We show that complete transgenes can be made and inserted into our split-selection safe harbor locations starting from PCR products, providing a clone-free and molecular-validation-free strategy for single-copy transgene integration. Overall, this combination of approaches provides an economical and rapid system for generating highly reproducible complex transgenics in C. elegans.