Manuel Ares

Purification of RNA using TRIzol (TRI reagent).

TRIzol solubilization and extraction is a relatively recently developed general method for deproteinizing RNA. This method is particularly advantageous in situations where cells or tissues are enriched for endogenous RNases or when separation of cytoplasmic RNA from nuclear RNA is impractical. TRIzol (or TRI Reagent) is a monophasic solution of phenol and guanidinium isothiocyanate that simultaneously solubilizes biological material and denatures protein. After solubilization, the addition of chloroform causes phase separation (much like extraction with phenol:chloroform:isoamyl alcohol), where protein is extracted to the organic phase, DNA resolves at the interface, and RNA remains in the aqueous phase. Therefore, RNA, DNA, and protein can be purified from a single sample (hence, the name TRIzol). TRIzol extraction is also an effective method for isolating small RNAs, such as microRNAs, piwi-associated RNAs, or endogeneous, small interfering RNAs. However, TRIzol is expensive and RNA pellets can be difficult to resuspend. Thus, the use of TRIzol is not recommend when regular phenol extraction is practical.

Isolation of Total RNA from Yeast Cell Cultures

This article describes two procedures for isolating total RNA from yeast cell cultures. The first allows the convenient isolation of total RNA from early log-phase cultures (vegetative cells). RNA isolated in this way is intact and sufficiently pure for use in microarray experiments, primer extension, and RNase protection mapping. With additional treatment to remove contaminating genomic DNA, the preparation is suitable for reverse transcription-polymerase chain reaction (RT-PCR), quantitative PCR (qPCR), cDNA library construction, high-throughput sequencing of RNA, or other manipulations. However, compared to vegetative cells, the isolation of RNA from cells late in meiosis (asci and ascospores) requires additional effort. This is because a tough cell wall composed of heavily cross-linked polysaccharides and proteins is built around the four spores during meiosis and ascospore development. Therefore, an alternative protocol is presented for extracting RNA from cells late in meiosis. This alternative may also be preferable for cells from stationary cultures or from yeast strains and other fungal species isolated from the environment.

Polyacrylamide gel electrophoresis of RNA

Perhaps the most important and certainly the most often used technique in RNA analysis is gel electrophoresis. This technique is generally applicable for RNA detection, quantification, purification by size, and quality assessment. Because RNAs are negatively charged, they migrate toward the anode in the presence of electric current. The gel acts as a sieve to selectively impede the migration of the RNA in proportion to its mass, given that its mass is generally proportional to its charge. Because mass is approximately related to chain length, the length of an RNA is more generally determined by its migration. In addition, topology (i.e., circularity) can affect migration, making RNAs appear longer on the gel than they actually are. Gels are used in a wide variety of techniques, including Northern blotting, primer extension, footprinting, and analyzing processing reactions. They are invaluable as preparative and fractionating tools. There are two common types of gel: polyacrylamide and agarose. For most applications, denaturing acrylamide gels are most appropriate. These gels are extremely versatile and can resolve RNAs from ~600 to </=20 nucleotides (nt). In certain circumstances, e.g., resolving different conformers of RNAs or RNA-protein complexes, native gels are appropriate. The only disadvantage to acrylamide gels is that they are not suitable for analyzing large RNAs (> or =600 nt); for such applications, agarose gels are preferred. This protocol describes how to prepare, load, and run polyacrylamide gels for RNA analysis.

Preparation of Cytoplasmic and Nuclear RNA from Tissue Culture Cells

It often is desirable to prefractionate RNA before analysis. Ordinarily, this can only be done with tissue culture cells, although it is possible to isolate nuclei and cytoplasm from certain soft tissues such as liver and white blood cells. This protocol describes a method for separating nuclei from the cytoplasm that can be used for many tissue culture types. This procedure also is useful for cells grown in suspension or for adherent cells. The procedure relies on swelling in hypotonic buffer, subsequent gentle homogenization, and centrifugation. This method is not appropriate for material (e.g., bacteria, yeast) that has high intrinsic RNase activity, or tissues that are difficult to solubilize, such as muscle tissue or plant material.

Nondenaturing Agarose Gel Electrophoresis of RNA

INTRODUCTION Perhaps the most important and certainly the most often used technique in RNA analysis is gel electrophoresis. Because RNAs are negatively charged, they migrate toward the anode in the presence of electric current. The gel acts as a sieve to selectively impede the migration of the RNA in proportion to its mass, given that its mass is generally proportional to its charge. Because mass is approximately related to chain length, the length of an RNA is more generally determined by its migration. In addition, topology (i.e., circularity) can affect migration, making RNAs appear longer on the gel than they actually are. There are two common types of gel: polyacrylamide and agarose. For most applications involving RNAs of < or =600 nucleotides, denaturing acrylamide gels are most appropriate. In contrast, agarose gels are generally used to analyze RNAs of > or =600 nucleotides, and are especially useful for analysis of mRNAs (e.g., by Northern blotting). RNA analysis on agarose gels is essentially identical to DNA analysis (except that the gel boxes used must be dedicated to RNA work or to other ribonuclease-free work). Here we describe the use of straightforward Tris borate, EDTA (TBE) gels for routine analysis. These gels are appropriate for determining the quantity and integrity of RNA before using it for other applications. This procedure should not be used to determine size with accuracy, because the RNA will not remain in its extended state throughout the run.

Purification of RNA by SDS Solubilization and Phenol Extraction

This protocol describes a method for RNA purification by sodium dodecyl sulfate (SDS) solubilization and phenol extraction. It is of wide utility and is used routinely to deproteinize RNAs in biological material that has been solubilized in SDS, an ionic detergent that dissolves membranes, disrupts protein-nucleic acid interactions, and inactivates ribonucleases. Once solubilized, addition of phenol or phenol:chloroform:isoamyl alcohol (PCA) completely denatures the protein, and it becomes insoluble in aqueous solution. PCA extraction is the method of choice for preparing cytoplasmic RNA from tissue culture cells or in any other situation (e.g., enzyme reactions) where solubilization in SDS is easily achievable.

Bacterial RNA Isolation

In this bacterial RNA isolation protocol, an RNA-protective treatment is followed by lysozyme digestion of the peptidoglycan component of the cell wall. EDTA promotes the loss of the outer membrane of Gram-negative bacteria and allows the lysozyme better access to the peptidoglycan. Cells begin to lyse during digestion in hypotonic lysozyme buffer and lysis is completed by sodium dodecyl sulfate (SDS) and hot phenol:chloroform:isoamyl alcohol (PCA) extraction. SDS and hot phenol disrupt membranes, denature protein (including RNase), and strip proteins from RNA. The separation of the organic phase from the aqueous phase is achieved using Phase Lock Gel, an inert material with a density intermediate between the organic and aqueous samples. The sample is split into three phases: from bottom to top, these are phenol and chloroform (organic phase), the inert gel with the interface material, and the aqueous phase with the RNA. The gel acts as a physical barrier between the sample and the organic phase plus interface. Following organic extraction, the RNA is concentrated by ethanol precipitation.

Guidelines for the use of RNA purification kits.

INTRODUCTIONnWith the proliferation of researchers investigating various aspects of RNA biology has come a corresponding proliferation of commercially available kits for RNA purification. Some of these kits have specialized uses and applications, and it is not always possible to simply mix and match the different protocols. Although the instructions are often written with a minimum of specifics concerning the chemical basis for the separation characteristics that the kits use, the competent researcher will want to understand these important features. Unfortunately, commercial sources work hard to hide the specifics of their methods. Fortunately, patent documents are publicly available, and the government mandates material safety data disclosures of the composition of at least those components that represent a threat to environmental health and safety. Thus, it is possible to infer many aspects of such proprietary materials, which in most cases are only slightly and unimportantly modified from published techniques. We do not describe in detail the specific steps involved in the use of particular kits; they are detailed in the literature that comes with each kit and their components (e.g., proprietary buffers). Instead, we detail some advantages and disadvantages of using RNA purification kits.

Methods for Processing High-Throughput RNA Sequencing Data

High-throughput sequencing (HTS) methods for analyzing RNA populations (RNA-Seq) are gaining rapid application to many experimental situations. The steps in an RNA-Seq experiment require thought and planning, especially because the expense in time and materials is currently higher and the protocols are far less routine than those used for other high-throughput methods, such as microarrays. As always, good experimental design will make analysis and interpretation easier. Having a clear biological question, an idea about the best way to do the experiment, and an understanding of the number of replicates needed will make the entire process more satisfying. Whether the goal is capturing transcriptome complexity from a tissue or identifying small fragments of RNA cross-linked to a protein of interest, conversion of the RNA to cDNA followed by direct sequencing using the latest methods is a developing practice, with new technical modifications and applications appearing every day. Even more rapid are the development and improvement of methods for analysis of the very large amounts of data that arrive at the end of an RNA-Seq experiment, making considerations regarding reproducibility, validation, visualization, and interpretation increasingly important. This introduction is designed to review and emphasize a pathway of analysis from experimental design through data presentation that is likely to be successful, with the recognition that better methods are right around the corner.

Fragmentation of Whole-Transcriptome RNA Using E. coli RNase III

High-throughput sequencing (HTS) methods can provide short sequence reads for many millions of individual molecules in a sample, allowing the use of sequencing to measure the abundance of RNA molecules. To quantify the amount of a particular sequence in a sample of large RNAs (e.g., mRNAs), it is important to fragment the RNA into short pieces that can be ligated to oligonucleotides that allow polymerase chain reaction (PCR) amplification and sequencing. The most desired end structure of RNA for such ligation steps is a 5 phosphate and a 3 OH. Thus, enzymes that leave these groups after cleavage are of particular utility, avoiding the need to dephosphorylate the 3 end with phosphatases or phosphorylate the 5 end with kinase before proceeding. One such enzyme, RNase III, is widely available. Although it primarily cuts duplex RNA, this specificity is salt- and concentration-dependent, and many RNAs that lack strong extended duplexes are nonetheless susceptible to cleavage at many spots. RNA fragmentation by RNase III does not seem to grossly affect the distribution of RNA sequencing reads. Thus, it has become a standard method for creating nominally representative pools of transcriptome sequences with 5 phosphates and 3 OH for library construction. Three steps in preparing fragmented transcriptome RNA for sequencing library construction are described here: (1) fragmenting the RNA with RNase III to the extent that ~60-100-nucleotide fragments are created, (2) purifying the RNA from the RNase III reaction, and (3) analyzing the digestion products for their suitability in library production.