Activity

Euglena gracilis, a unicellular phytoflagellate microalga, is a promising biomaterial for foods, feeds, and biofuels. However, targeted mutagenesis in this species has been a long-standing challenge. We recently developed a transgene-free, highly efficient, genome editing method for E. gracilis using CRISPR/Cas9 ribonucleoproteins (RNPs). Our method achieved mutagenesis rates of approximately 80% or more through an electroporation-based direct delivery of Cas9 RNPs. Therefore, this method is suitable for basic research and industrial applications, such as the breeding of Euglena. For complete details on the use and execution of this protocol, please refer to Nomura et al. (2019).Accumulating evidence indicates that the immune system is regulated not only by immune cells but also by stromal cells in the tissue microenvironment. Characterization of non-hematopoietic cells has not been performed in depth, since markers of the subsets are limited. Recent advances of single-cell technology allow researchers to characterize comprehensively the heterogeneity of stromal cells in an unbiased manner. In this article, we provide step-by-step protocols for cell preparation for single-cell RNA sequencing to characterize the heterogeneity of stroma in human lymph nodes. For complete details on the use and execution of this protocol, please refer to Takeda et al. (2019).This protocol describes the isolation, handling, culture of, and experiments with human colon stem cell organoids in the context of cystic fibrosis (CF). In human colon organoids, the function of cystic fibrosis transmembrane conductance regulator (CFTR) protein and its rescue by CFTR modulators can be quantified using the forskolin-induced swelling assay. Implementation procedures and validation experiments are described for six CF human colon organoid lines, and representative CFTR genotypes are tested for basal CFTR function and response to CFTR-modulating drugs. For complete details on the use and execution of this protocol, please refer to Dekkers et al (2016) and Berkers and van Mourik (2019).Exploring the biological functions of the human glycome is highly challenging given its tremendous structural diversity. We have developed stable libraries of isogenic HEK293 cells with loss or gain of glycosylation features that together form the cell-based glycan array, a self-renewable resource for the display of the human glycome in the natural context. This protocol describes the use of the cell-based glycan array for dissection of molecular interactions and biological functions of glycans using a wide range of biological assays. For complete details on the use and execution of this protocol, please refer to (Narimatsu et al., 2019).De novo identification of chromatin interactors can reveal unexpected pathways relevant to physiology and human disease. Inspired by the DNA mediated chromatin pull-down (Dm-ChP) technology (also known as iPOND [isolation of proteins on nascent DNA]) for the proteomic characterization of nascent DNA, we have recently reported a new experimental protocol that allows for the identification of proteins on total DNA (iPOTD) for bulk chromatome profiling and de novo identification of chromatin-bound proteins. Here, we detail a step-by-step protocol to survey the cellular chromatin-bound proteome in a simple, robust, and unbiased manner. For complete details on the use and execution of this protocol, please refer to Aranda et al. (2019).This protocol introduces the SuperSTORM technique, combining stochastic optical reconstruction microscopy (STORM) and molecular modeling. SuperSTORM is optimized for acquiring and processing STORM images of neutrophil integrins but can be used for any cell-surface molecule with known structure and antibody-binding site(s). SuperSTORM identifies molecular cut-offs for eliminating multiple blinks of STORM imaging, determines colocalization, identifies clusters, and reveals molecular orientations and distributions. This protocol extends STORM imaging to cells in microfluidic systems. Improved resolution is achieved by using biomolecule-inherent parameters. For complete information on the generation and use of this protocol, please refer to the paper by Fan et al. (2019).This protocol is a procedure for establishment and culture of cancer and non-cancer organoids using tissues from biliary tract carcinoma (BTC) patients. These BTC organoids can be used for various biological analyses and drug screening. One challenge in establishing and culturing BTC organoids is non-cancer cells contaminating surgically resected tumor tissues form organoids concurrently with cancer organoids. Careful validation that the established organoids are cancer-derived is important. For complete details on the use and generation of this protocol, please refer to Saito et al. (2019) in the journal Cell Reports.We describe an optimized smFISH protocol for the intact pancreas. The protocol is adapted from Lyubimova et al. (2013), a generic tissue smFISH protocol that works for most tissues but not the pancreas. The main changes implemented include increasing the period of mRNA denaturation from 5 min to at least 3 h and increasing formamide concentrations from 10% to 30%. These modifications yield sensitive single mRNA visualization that is comparable to those achieved in other tissues using the standard protocol. For complete details on the use and execution of this protocol, please refer to Farack et al., 2018, Farack et al., 2019.DNA-FISH remains the method of choice to visualize genomic regions in situ ranging from a single locus to entire chromosomes. Current methods to generate probes rely on expensive kits that vary in labeling efficiency and are limited by the size and/or amount of starting material and by the choice of fluorophores. Here we describe a protocol to prepare inexpensive ($20) DNA-FISH probes using an isothermal polymerase, incorporating labeled nucleotides while amplifying minute amounts of any template (PCR fragments/BAC/YAC/fosmids). For complete details on the use and execution of this protocol, please refer to Grosmaire et al. (2019) and Sharma et al. Lenalidomide hemihydrate manufacturer (2014).