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RNA sequencing (RNA-Seq) has emerged as a powerful and versatile tool for the comprehensive analysis of transcriptomes and has been widely used to investigate gene expression, copy number variation, alternative splicing, and novel transcript discovery. This chapter outlines the methodology for conducting short-read RNA-Seq, starting from RNA enrichment to library preparation and sequencing. Throughout the chapter, practical tips and best practices are provided to guide researchers in order to optimize each step of the RNA-Seq workflow. Multiple quality control steps throughout the workflow that are critical to obtain high-quality RNA-Seq data are also discussed., (© 2024. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

PacBio long-read sequencing is a third-generation technology that generates long reads up to 20 kilobases (kb), unlike short-read sequencing instruments that produce up to 600 bases. Long-read sequencing is particularly advantageous in higher organisms, such as humans and plants, where repetitive regions in the genome are more abundant. The PacBio long-read sequencing uses a single molecule, real-time approach where the SMRT cells contain several zero-mode waveguides (ZMWs). Each ZMW contains a single DNA molecule bound by a DNA polymerase. All ZMWs are flushed with deoxy nucleotides with a fluorophore specific to each nucleotide. As the sequencing proceeds, the detector detects the wavelength of the fluorescence and the nucleotides are read in real-time. This chapter describes the sample and library preparation for PacBio long-read sequencing for grapevine., (© 2024. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

The article presents the several steps to be performed on a plant, fungal, insect, or soil sample to obtain DNA sequences for DNA barcode analysis. The chapter begins with a description of sample preparation including procedures for cleaning and proceeds to DNA extraction with methods adapted for the specific type of sample. Next, DNA quantification is described so the proper amount is used for the amplification of the selected barcode regions. Information is provided for reaction mixes and amplification conditions for several referenced barcode primer pairs tuned for the individual sample of interest. This is followed by a description of procedures to access the success of amplification, cleanup, and quantification of the product ready for either Sanger sequencing or library preparation for massive parallel sequencing (MPS). Finally, procedures are provided for Sanger sequencing, library preparation, and MPS sequencing. The chapter provides several references of barcode regions for different sample types., (© 2024. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Modern high-throughput genomic testing using next-generation sequencing (NGS) has led to a significant increase in the successful diagnosis of rare genetic disorders. Recent advances in NGS tools and techniques have led to accurate and timely diagnosis of a large proportion of genetic diseases by finding sequence variations in clinical samples. One of the NGS techniques, exome sequencing (ES), is considered as a powerful and easily approachable method for genetic disorders in terms of rapid and cost-effective diagnostic yields. In this chapter, we describe an overview of whole exome sequencing (ES) in the context of experimental and analytical methodologies. Approaches to ES include sequencing capture technique, quality control processes at various stages of sequencing analysis, exome data filtering strategy that incorporates both primary and secondary filtering, and prioritization of candidate variants in diagnosing genetic diseases., (© 2024. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Long read Nanopore sequencing can be utilised to determine the quality and accuracy of genetically engineered changes in animals, which often produce heterogenous samples. The protocol presented in this chapter can be used for a range of both low and high throughput sequencing applications. DNA must be repaired, barcoded and ligated to sequencing adapters prior to sequencing. Quality of sequencing data produced is dependent on stringent adherence to the protocol. However, nanopore sequencing is a fast moving field, therefore it is worth considering using the most up to date chemistry available., (© 2023. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Structural variant detection by next-generation sequencing (NGS) methods have a higher molecular resolution than conventional cytogenetic techniques (Aypar et al., Eur J Haematol 102(1):87-96, 2019; Smadbeck et al., Blood Cancer J 9(12):103, 2019) and are particularly helpful in characterizing genomic rearrangements. Mate pair sequencing (MPseq) leverages a unique library preparation chemistry involving circularization of long DNA fragments, allowing for a unique application of paired-end sequencing of reads that are expected to map 2-5 kb apart in the genome. The unique orientation of the reads allows the user to estimate the location of breakpoints involved in a structural variant either within the sequenced reads or between the two reads. The precision of structural variant and copy number detection by this method allows for characterization of cryptic and complex rearrangements that may be otherwise undetectable by conventional cytogenetic methods (Singh et al., Leuk Lymphoma 60(5):1304-1307, 2019; Peterson et al., Blood Adv 3(8):1298-1302, 2019; Schultz et al., Leuk Lymphoma 61(4):975-978, 2020; Peterson et al., Mol Case Studies 5(2), 2019; Peterson et al., Mol Case Studies 5(3), 2019)., (© 2023. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Mitochondrial genomes (mtgenome) represent an important source of information for addressing fundamental evolutionary, phylogeographic, systematic, and ecological questions in marine organisms. In the last two decades the advent of high-throughput next-generation sequencing (NGS) has provided an unprecedented possibility to access large amount of genomic data and, as such, there has been a rapid growth in mtgenome resources and studies. In particular, NGS strategies represent a great advantage for investigating nonmodel marine organisms for which no or limited genomic resources are available. Here, we describe a routinely used standardized protocol to obtain mtgenome of nonmodel marine organisms by NGS. The protocol is composed of five main steps, including DNA extraction, DNA fragmentation, library preparation, high-throughput sequencing, and bioinformatic analyses. Each of the first three steps is followed by size/quality and concentration validations. The advantages of the described protocol rely on the assumption that no a priori information on mtgenome of the studied organism is needed and on its versatility as researchers may choose several kits for DNA extraction and library preparation and adopt different methods for DNA fragmentation depending on their needs, experience, and suppliers., (© 2022. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

The study of small RNAs (sRNAs) by next-generation sequencing (NGS) is challenged by bias issues during library preparation. Several types of sRNAs such as plant microRNAs (miRNAs) carry a 2'-O-methyl (2'-OMe) modification at their 3' terminal nucleotide. This modification adds another level of difficulty as it inhibits 3' adapter ligation. We previously demonstrated that modified versions of the "TruSeq (TS)" protocol have less bias and an improved detection of 2'-OMe RNAs. Here we describe in detail protocol "TS5," which showed the best overall performance. We also provide guidelines for bioinformatics analysis of the sequencing data.

Next-generation sequencing (NGS) of immunoglobulin (IG) and T cell receptor (TR) rearrangements represents a modern alternative to classical RQ-PCR-based minimal residual disease (MRD) detection. The same primer sets and conditions can be used for all patients, which is undoubtedly one of the most important benefits of NGS, not only reducing the labor required to perform the analysis but also enabling the assay to comply with the upcoming EU IVD regulation. So far, only one standardized academic protocol for this task has been published, developed, and validated within the EuroClonality-NGS working group. In this chapter we describe the materials and methods for amplicon library preparation for sequencing on Illumina MiSeq, and the bioinformatic pipeline for this protocol.

Enhancers are transcribed by RNA polymerase II (Pol II). In order to study the regulation of enhancer transcription and its function in target gene control, methods are required that track genome transcription with high precision in vivo. Here, we provide step-by-step guidance for performing native elongating transcript sequencing (NET-Seq) in mammalian cells. NET-Seq allows quantitative measurements of transcription genome-wide, including enhancer transcription, with single-nucleotide and DNA strand resolution. The approach consists of capturing and efficiently converting the 3'-ends of the nascent RNA into a sequencing library followed by next-generation sequencing and computational data analysis. The protocol includes quality control measurements to monitor the success of the main steps. Following this protocol, a NET-Seq library is obtained within 5 days., (© 2021. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Extracellular RNAs (exRNAs) are secreted by nearly all cell types and are now known to play multiple physiological roles. Human plasma, a readily available sample for biomedical analysis, was reported to contain various subpopulations of exRNA, some of which are most likely components of plasma ribonucleoproteins (RNPs), while others are encapsulated into extracellular vesicles (EVs) of different size, origin, and composition. Unbiased analysis of exRNA composition can be performed with prefractionation of plasma exRNA followed by library preparation, sequencing, and bioinformatics analysis. In addition to "mature," adaptor ligation-competent RNA species (5'-P/3'-OH), human plasma contains a substantial proportion of degraded RNA fragments, featuring 5'-OH/3'-P or cyclophosphate extremities, which can be made competent for ligation using appropriate treatment. Polyethylene glycol (PEG)-based precipitation kits for EV isolation yield a fraction that is highly contaminated by large RNPs and EV-associated RNAs. Purer EV preparations are obtained by using Proteinase K and RNase A treatment, as well as by size-exclusion chromatography (SEC).

RNA sequencing (RNA-seq) is an integral tool in immunogenomics, allowing for interrogation of the transcriptome of a tumor and its microenvironment. Analytical methods to deconstruct the genomics data can then be applied to infer gene expression patterns associated with the presence of various immunocyte populations. High quality RNA-seq is possible from formalin-fixed, paraffin-embedded (FFPE), fresh-frozen, and fresh tissue, with a wide variety of sequencing library preparation methods, sequencing platforms, and downstream bioinformatics analyses currently available. Selection of an appropriate library preparation method is largely determined by tissue type, quality of RNA, and quantity of RNA. Downstream of sequencing, many analyses can be applied to the data, including differential gene expression analysis, immune gene signature analysis, gene pathway analysis, T/B-cell receptor inference, HLA inference, and viral transcript quantification. In this chapter, we will describe our workflow for RNA-seq from bulk tissue to evaluable data, including extraction of RNA, library preparation methods, sequencing of libraries, alignment and quality assurance of data, and initial downstream analyses of RNA-seq data to extract relevant immunogenomics features. Systems biology methods that draw additional insights by integrating these features are covered further in Chapters 28 - 30 .

High-throughput next generation sequencing karyotyping has emerged as a powerful tool for the detection of genomic heterogeneity in normal tissues and cancers. Here we describe a single-cell whole genome sequencing (scWGS) platform to assess whole-chromosome aneuploidy, structural aneuploidies involving only chromosome fragments and more local small copy number alterations in individual cells. We provide a detailed protocol for the isolation, library preparation, low coverage sequencing and data analysis of single cells. Since our approach does not involve a whole-genome preamplification step, our method allows for acquisition of reliable high-resolution single-cell copy number profiles. Moreover, the protocol allows multiplexing of 384 single-cell libraries in one sequencing run, thereby significantly reducing sequencing costs and can be completed in 3-4 days starting from single cell isolation to analysis of sequencing data.

The analysis of single-nucleotide polymorphisms (SNPs) has proven to be advantageous for addressing variation within samples of highly degraded or low-quality DNA samples. This is because only short fragments need to be amplified to analyze SNPs, and this can be achieved by multiplex PCR. Here, we present a sensitive method for the targeted sequencing of SNP loci that requires only small amounts of template DNA. The approach combines multiplex amplification of very short fragments covering SNP positions followed by sample barcoding and next-generation sequencing. This method allows generation of data from large sample sets of poorly preserved specimens, such as fossil remains, forensic samples, and museum specimens. The approach is cost-effective, rapid, and applicable to forensics, population genetics, and phylogenetic research questions.

Genomic library preparation from highly degraded DNA is more efficient when library molecules are prepared separately from the complementary strands of DNA fragments. We describe a protocol in which libraries are constructed from single DNA strands in a three-step procedure: single-stranded ligation of the first adapter with T4 DNA ligase in the presence of a splinter oligonucleotide, copying of the DNA strand with a proofreading polymerase, and blunt-end ligation of the second double-stranded adapter with T4 DNA ligase.

Single-cell technologies have emerged as advanced tools to study various biological processes that demand the single cell resolution. To detect subtle heterogeneity in the transcriptome, high accuracy and sensitivity are still desired for single-cell RNA-seq. We describe here multiple annealing and dC-tailing-based quantitative single-cell RNA-seq (MATQ-seq) with ~90% capture efficiency. In addition, MATQ-seq is a total RNA assay allowing for detection of nonpolyadenylated transcripts.

Exome capture is a reduced representation approach that selectively captures sequence from only the gene-bearing regions of a genome. It is based on probes targeted at these regions and, compared with whole genome shotgun sequencing, leads to a significant reduction in cost and data processing effort while still providing insights into the most relevant part of a genome. An exome capture array for barley was released in 2013 and this has opened the door to numerous studies that have put this technology to good use. In this chapter we detail the laboratory protocols required for enrichment and sequencing, and provide detailed step-by-step instructions for the bioinformatics analysis of the resulting data.

Single-cell RNA-seq technology allows for the identification of heterogeneous cell populations, measures stochastic gene expressions, and identifies highly variable genes. Thus, with this technology it is possible to identify relevant pathways involved in development or in disease progression. Herein, we describe a protocol to capture and process single-cell transcriptomes that will be used for RNA sequencing. This chapter discusses the use of the Fluidigm C1 System and Integrated Fluidic Circuit microfluidics system, TapeStation 4200, SMART-Seq v4, Nextera XT Library Preparation Kit, and AMPure XP beads.

In this chapter, we describe a method for making Illumina-compatible sequencing libraries from RNA. This protocol can be used for standard RNAseq analysis for detecting differentially expressed genes. In addition, this protocol is ideally suited for adapting to RIPseq, 5'-RACE, RNA structural probing, nascent RNA sequencing, and other protocols where polymerase termination sites need to be profiled. The utilization of solid-phase bead chemistries facilitates simple workflow and efficient library yields.

Whole exome sequencing (WES) is a DNA sequencing strategy that provides a survey of base substitutions across coding genomic locations and other regions of interest. As the coding portion of the genome encompasses only 1-2% of the entire genome, this approach represents a more cost-effective strategy to detect DNA alterations that may alter protein function, compared to whole genome sequencing. Although the research community has and is currently delineating the functional implications of sequence changes in noncoding regions of the genome, WES is a currently available assay that provides valuable information for both discovery research and precision medicine applications. In this chapter, we present a WES library preparation protocol using the KAPA Hyper Prep Kit with Agilent SureSelect Human All Exon V5+UTR probes that demonstrates high DNA-to-library conversion efficiency for sequencing on the Illumina HiSeq platform.

Reduced representation bisulfite sequencing (RRBS) is one of the most comprehensive yet economic ways of mapping whole genome DNA-methylation. Here, we have substantially modified the RRBS protocol by combining end-repair and A-tailing steps, and by introducing a bead-based method for rapid and easy size selection of the library molecules. The method has been optimized for myeloma clinical samples, where the input DNA concentration can be as low as 100 ng. The method developed can be accomplished in 3 days, including the initial overnight MspI enzyme digestion. Although the protocol has been optimized in myeloma samples, it is broadly applicable to any clinical sample, which is restricted by very low input DNA concentrations.

Whole genome wide analysis of transcription using RNA-Seq methods is a powerful way to elucidate differential expression of gene features in bacteria across different conditions as well as for discovering previously exotic RNA species. Indeed, RNA sequencing has revolutionized the study of bacterial transcription with the diversity and quantity of small noncoding RNA elements that have been found and its ability to clearly define operons, promoters , and terminators . We discuss our experience with applying RNA sequencing technology to analyzing the lytic cycle, including extraction, processing, and a guide to the customized statistical analysis necessary for analyzing differential host and phage transcription.

Next-generation small RNA sequencing is a valuable tool which is increasing our knowledge regarding small noncoding RNAs and their function in regulating genetic information. Library preparation protocols for small RNA have thus far been restricted due to higher RNA input requirements (>10 ng), long workflows, and tedious manual gel purifications. Small RNA library preparation methods focus largely on the prevention or depletion of a side product known as adapter dimer that tends to dominate the reaction. Adapter dimer is the ligation of two adapters to one another without an intervening library RNA insert or any useful sequencing information. The amplification of this side reaction is favored over the amplification of tagged library since it is shorter. The small size discrepancy between these two species makes separation and purification of the tagged library very difficult. Adapter dimer hinders the use of low input samples and the ability to automate the workflow so we introduce an improved library preparation protocol which uses chemically modified adapters (CleanTag) to significantly reduce the adapter dimer. CleanTag small RNA library preparation workflow decreases adapter dimer to allow for ultra-low input samples (down to approx. 10 pg total RNA), elimination of the gel purification step, and automation. We demonstrate how to carry out this streamlined protocol to improve NGS data quality and allow for the use of sample types with limited RNA material.

Next-generation DNA sequencing (NGS) technologies have made generating genomic sequence for organisms of interest affordable and commonplace. However, NGS platforms and analysis software are generally tuned to be used on large and complex genomes or metagenomic samples. Determining the complete genome sequence of a single bacteriophage requires a somewhat different perspective, workflow, and sensitivity to the nature of phages. Because phage genomes consist of mostly coding regions (see Pope/Jacobs-Sera chapter), a very high standard should be adopted when completing these genomes so that the subsequent steps of annotation and analysis are not sabotaged by sequencing errors. While read quality and assembly algorithms have continued to improve, achieving this standard still requires a significant amount of human oversight and expertise. This chapter describes our workflow for sequencing, assembling, and finishing phage genomes to a high standard by the NGS platforms Illumina, Ion Torrent, and 454.

Chromatin immunoprecipitation (ChIP) is a widely used method to map the position of DNA-binding proteins such as histones and transcription factors (TFs) upon their interaction with particular regions of the genome. To examine the genomic distribution of a TF in specific cell types in response to a change in nitrogen concentration, we developed a micro-ChIP (μChIP) protocol that requires only ~5000 Arabidopsis cells transiently expressing the Arabidopsis TF Basic Leucine Zipper 1 (bZIP1) fused to the glucocorticoid receptor (GR) domain that mediates nuclear import in the presence of dexamethasone. The DNA fragments obtained from the immunoprecipitation of bZIP1-DNA complexes were analyzed by next-generation sequencing (ChIP-seq), which helped uncover genome-wide associations between a bZIP1 and its targets in plant cells upon fluctuations in nitrogen availability.

Serine protease inhibitors, serpins, can have profound effects on many systems in the body including immune defense systems. The microbiome, specifically the gut and lung bacterial microbiota, is now known, under some conditions, to alter immune defenses. DNA library preparation for microbiome studies is a procedure that prepares microbial genomic DNA to be sequenced in next-generation sequencing platforms. The construction involves a PCR reaction that will amplify the 16S rRNA gene and will incorporate a specific index and adaptors to the fragments. After confirmation of the product amplification by gel electrophoresis, samples will be later normalized to the same DNA amount of 240 ng. Final concentration of the library is validated by quantitative PCR (qPCR).Here we describe methods to analyze changes in the microbiome after treatment with immune-modulating agents, specifically serpins.

Chromatin immunoprecipitation coupled with high-throughput, next-generation DNA sequencing (ChIP-seq) has enabled researchers to establish the genome-wide patterns of chromatin modifications and binding of chromatin-associated proteins. Well-established protocols produce robust ChIP-seq data for many proteins by sequencing the DNA obtained following immunoprecipitation of fragmented chromatin using a wide range of specific antibodies. In general, the quality of these data mainly depends on the specificity and avidity of the antibody used. However, even using optimal antibodies, ChIP-seq can become more challenging when the protein associates with chromatin via protein-protein interactions rather than directly binding DNA. An example of such a protein is the alpha-thalassaemia mental retardation X-linked (ATRX) protein; a chromatin remodeler that associates with the histone chaperone DAXX, in the deposition of the replication-independent histone variant H3.3 and plays an important role in maintaining chromatin integrity. Inherited mutations of ATRX cause syndromal mental retardation (ATR-X Syndrome) whereas acquired mutations are associated with myelodysplasia, acute myeloid leukemia (ATMDS syndrome), and a range of solid tumors. Therefore, high quality ChIP-seq data have been needed to analyze the genome-wide distribution of ATRX, to advance our understanding of its normal role and to comprehend how mutations contribute to human disease. Here, we describe an optimized ChIP-seq protocol for ATRX which can also be used to produce high quality data sets for other challenging proteins which are indirectly associated with DNA and complement the ChIP-seq toolkit for genome-wide analyses of histone chaperon complexes and associated chromatin remodelers. Although not a focus of this chapter, we will also provide some insight for the analysis of the large dataset generated by ChIP-seq. Even though this protocol has been fully optimized for ATRX, it should also provide guidance for efficient ChIP-seq analysis, using the appropriate antibodies, for other proteins interacting indirectly with DNA.

MinION is a small form factor sequencer recently retailed by Oxford Nanopore technologies. This lighter-sized USB3.0-interfaced device uses innovative nanotechnology to generate extra-long reads from libraries prepared using only standard molecular biology lab equipment. The flexibility and the portability of the platform makes it ideal for point-of-interest and real-time surveillance applications. However, MinION's limited capacity is not enough for the study of specific targets within larger genomes. Apart from just PCR-amplifying regions of interest, the capture of long reads spanning the edges of known-unknown genomic regions is of great importance for structural studies, such as the identification of mobile elements' integrations sites, bridging over low complexity repetitive regions etc.In this study, using MinION-kit-included and commercially available reagents, we have developed an easy and versatile wet-lab procedure for the targeted enrichment of MinION libraries, capturing DNA fragments of interest before the ligation of the sensitive MinION sequencing-adapters. This method allows for simultaneous target-enrichment and barcode-multiplexing of up to 12 libraries, which can be loaded in the same sequencing run.

Identifying gene expression changes mediated by signaling pathways is necessary to determine mechanisms that cause phenotypic change. Recent advances in next-generation sequencing and informatic pipelines have streamlined the ability for laboratories to create and analyze transcriptomic data. Here, we describe the preparation of samples and transcriptomic analysis in order to determine gene expression programs regulated by RAS/ERK signaling.

Developmental genomics is a rapidly growing field, and high-quality genomes are a useful foundation for comparative developmental studies. A high-quality genome forms an essential reference onto which the data from numerous assays and experiments, including ChIP-seq, ATAC-seq, and RNA-seq, can be mapped. A genome also streamlines and simplifies the development of primers used to amplify putative regulatory regions for enhancer screens, cDNA probes for in situ hybridization, microRNAs (miRNAs) or short hairpin RNAs (shRNA) for RNA interference (RNAi) knockdowns, mRNAs for misexpression studies, and even guide RNAs (gRNAs) for CRISPR knockouts. Finally, much can be gleaned from comparative genomics alone, including the identification of highly conserved putative regulatory regions. This chapter provides an overview of laboratory and bioinformatics protocols for DNA extraction, library preparation, library quantification, and genome assembly, from fresh or frozen tissue to a draft avian genome. Generating a high-quality draft genome can provide a developmental research group with excellent resources for their study organism, opening the doors to many additional assays and experiments.

ARGONAUTE (AGO) proteins function in small RNA (sRNA)-based RNA silencing pathways to regulate gene expression and control invading nucleic acids. In posttranscriptional RNA silencing pathways, plant AGOs associate with sRNAs to interact with highly sequence-complementary target RNAs. Once the AGO-sRNA-target RNA ternary complex is formed, target RNA is typically repressed through AGO-mediated cleavage or through other cleavage-independent mechanisms. The universe of sRNAs associating with diverse plant AGOs has been determined though AGO immunoprecipitation (IP) and high-throughput sequencing of co-immunoprecipitated sRNAs. To better understand the biological functions of AGO-sRNA complexes, it is crucial to identify the repertoire of target RNAs they regulate. Here I present a detailed AGO-RNA IP followed by high-throughput sequencing (AGO RIP-Seq) methodology for the isolation of AGO ternary complexes from plant tissues and the high-throughput sequencing of AGO-bound target RNAs. In particular, the protocol describes the IP of slicer-deficient hemagglutinin (HA)-tagged AGO proteins expressed in plant tissues, the isolation of AGO-bound RNAs, and the generation of target RNA libraries for high-throughput sequencing.

The nucleolus is a subcellular compartment with a key essential function in ribosome biogenesis. The nucleolus is rich in noncoding RNAs, mostly the ribosomal RNAs and small nucleolar RNAs. Surprisingly, also several miRNAs have been detected in the nucleolus, raising the question as to whether other small RNA species are present and functional in the nucleolus. We have developed a strategy for stepwise enrichment of nucleolar small RNAs from the total nucleolar RNA extracts and subsequent construction of nucleolar small RNA libraries which are suitable for deep sequencing. Our method successfully isolates the small RNA population from total RNAs and monitors the RNA quality in each step to ensure that small RNAs recovered represent the actual small RNA population in the nucleolus and not degradation products from larger RNAs. We have further applied this approach to characterize the distribution of small RNAs in different cellular compartments.