The genome of the dengue virus codes for a single polypeptide that yields three structural and seven non-structural (NS) proteins upon post-translational modifications. Among them, NS protein-3 (NS3) possesses protease activity, involved in the processing of the self-polypeptide and in the cleavage of host proteins. Identification and analysis of such host proteins as substrates of this protease facilitate the development of specific drugs. In vitro cleavage analysis has been applied, which requires homogeneously purified components. However, the expression and purification of both S3 and erythroid differentiation regulatory factor 1 (EDRF1) are difficult and unsuccessful on many occasions. EDRF1 was identified as an interacting protein of dengue virus protease (NS3). The amino acid sequence analysis indicates the presence of NS3 cleavage sites in this protein. As EDRF1 is a high-molecular-weight (~138 kDa) protein, it is difficult to express and purify the complete protein. In this protocol, we clone the domain of the EDRF1 protein (C-terminal end) containing the cleavage site and the NS3 into two different eukaryotic expression vectors containing different tags. These recombinant vectors are co-transfected into mammalian cells. The cell lysate is subjected to SDS-PAGE followed by western blotting with anti-tag antibodies. Data suggest the disappearance of the EDRF1 band in the lane co-transfected along with NS3 protease but present in the lane transfected with only EDRF1, suggesting EDRF1 as a novel substrate of NS3 protease. This protocol is useful in identifying the substrates of viral-encoded proteases using ex vivo conditions. Further, this protocol can be used to screen anti-protease molecules.

Key features

• This protocol requires the cloning of protease and substrate into two different eukaryotic expression vectors with different tags.

• Involves the transfection and co-transfection of both the above recombinant vectors individually and together.

• Involves western blotting of the same PVDF membrane containing total proteins of the cell lysate with two different antibodies.

• Does not require purified proteins for the analysis of cleavage of any suspected substrate by the protease.

Graphical overview

Mitochondria play decisive roles in bioenergetics and intracellular communication. These organelles contain a circular mitochondrial DNA (mtDNA) genome that is duplicated within one to two hours by a mitochondrial replisome, independently from the nuclear replisome. mtDNA stability is regulated in part at the level of mtDNA replication. Consequently, mutations in mitochondrial replisome components result in mtDNA instability and are associated with diverse disease phenotypes, including premature aging, aberrant cellular energetics, and developmental defects. The mechanisms ensuring mtDNA replication stability are not completely understood. Thus, there remains a need to develop tools to specifically and quantifiably examine mtDNA replication. To date, methods for labeling mtDNA have relied on prolonged exposures of 5′-bromo-2′-deoxyuridine (BrdU) or 5′-ethynyl-2′-deoxyuridine (EdU). However, labeling with these nucleoside analogs for a sufficiently short time in order to monitor nascent mtDNA replication, such as under two hours, does not produce signals suited for efficient or accurate quantitative analysis. The assay system described here, termed Mitochondrial Replication Assay (MIRA), utilizes proximity ligation assay (PLA) combined with EdU-coupled Click-IT chemistry to address this limitation, thereby enabling sensitive and quantitative analysis of nascent in situ mtDNA replication with single-cell resolution. This method can be further paired with conventional immunofluorescence (IF) for multi-parameter cell analysis. By enabling monitoring nascent mtDNA prior to the complete replication of the entire mtDNA genome, this new assay system allowed the discovery of a new mitochondrial stability pathway, mtDNA fork protection. Moreover, a modification in primary antibodies application allows the adaptation of our previously described in situ protein Interactions with nascent DNA Replication Forks (SIRF) for the detection of proteins of interest to nascent mtDNA replication forks on a single molecule level (mitoSIRF).

Graphical overview

Schematic overview of Mitochondrial Replication Assay (MIRA). 5′-ethynyl-2′-deoxyuridine (EdU; green) incorporated in DNA is tagged with biotin (blue) using Click-IT chemistry. Subsequent proximity ligation assay (PLA, pink circles) using antibodies against biotin allows the fluorescent tagging of the nascent EdU and amplification of the signal sufficient for visualization by standard immunofluorescence. PLA signals outside the nucleus denote mitochondrial DNA (mtDNA) signals. Ab, antibody. In in situ protein interactions with nascent DNA replication forks (mitoSIRF), one of the primary antibodies is directed against a protein of interest, while the other detects nascent biotinylated EdU, thus enabling in situ protein interactions with nascent mtDNA.

In the human cell cycle, complete replication of DNA is a fundamental process for the maintenance of genome integrity. Replication stress interfering with the progression of replication forks causes difficult-to-replicate regions to remain under-replicated until the onset of mitosis. In early mitosis, a homology-directed repair DNA synthesis, called mitotic DNA synthesis (MiDAS), is triggered to complete DNA replication. Here, we present a method to detect MiDAS in human U2OS 40-2-6 cells, in which repetitive lacO sequences integrated into the human chromosome evoke replication stress and concomitant incomplete replication of the lacO array. Immunostaining of BrdU and LacI proteins is applied for visualization of DNA synthesis in early mitosis and the lacO array, respectively. This protocol has been established to easily detect MiDAS at specific loci using only common immunostaining methods and may be optimized for the investigation of other difficult-to-replicate regions marked with site-specific binding proteins.

Ribosome profiling (Ribo-Seq) is a highly sensitive method to quantify ribosome occupancies along individual mRNAs on a genome-wide scale. Hereby, ribosome-protected fragments (= footprints) are generated by nuclease digestion, isolated, and sequenced together with the corresponding randomly fragmented input samples, to determine ribosome densities (RD). For library preparation, equal amounts of total RNA are used. Subsequently, all transcript fragments are subjected to linker ligation, cDNA synthesis, and PCR amplification. Importantly, the number of reads obtained for every transcript in input and footprint samples during sequencing depends on sequencing depth and library size, as well as the relative abundance of the transcript in the sample. However, the information pertaining to the absolute amount of input and footprint sequences is lost during sample preparation, hence ruling out any conclusion whether translation is generally suppressed or activated in one condition over the other. Therefore, the RD fold-changes determined for individual genes do not reflect absolute regulation, but have to be interpreted as relative to bulk mRNA translation. Here, we modified the original ribosome profiling protocol that was first established by Ingolia et al. (2009), by adding small amounts of yeast lysate to the mammalian lysates of interest as a spike-in. This allows us to not only detect changes in the RD of specific transcripts relative to each other, but also to simultaneously measure global differences in RD (normalized ribosome density values) between samples.

Graphic abstract:

Global changes in translation efficiency can be detected with polysome profiling, where the proportion of polysomal ribosomes is interpreted as a proxy for ribosome density (RD) on bulk mRNA. Ribo-Seq measures changes in RD of specific mRNAs relative to bulk mRNA. The addition of a yeast-lysate, as a spike-in for normalization of read counts, allows for an absolute measurement of changes in RD.

The COVID-19 pandemic requires mass screening to identify those infected for isolation and quarantine. Individually screening large populations for the novel pathogen, Severe Acute Respiratory Syndrome Coronavirus 2 (SARS-CoV-2), is costly and requires a lot of resources. Sample pooling methods improve the efficiency of mass screening and consume less reagents by increasing the capacity of testing and reducing the number of experiments performed, and are therefore especially suitable for under-developed countries with limited resources. Here, we propose a simple, reliable pooling strategy for COVID-19 testing using clinical nasopharyngeal (NP) and/or oropharyngeal (OP) swabs. The strategy includes the pooling of 10 NP/OP swabs for extraction and subsequent testing via quantitative real-time reverse transcription polymerase chain reaction (RT-qPCR), and may also be applied to the screening of other pathogens.

Maternal immune activation (MIA) is increasingly well appreciated as an environmental risk factor for some psychiatric disorders. Administration of proinflammatory compounds such as the synthetic double-stranded RNA molecule polyinosinic-polycytidylic acid (polyI:C) to pregnant rodents results in the release of proinflammatory cytokines in the maternal circulation. Various behavioural and brain changes are produced in the offspring that are associated with psychiatric disorders such as autism and schizophrenia. This protocol describes the steps necessary for inducing MIA in pregnant rat dams, which will allow for investigations into the mechanisms in the dam and offspring that mediate the long-term effects of exposure to inflammation while in utero. Increasing our understanding of these mechanisms may provide new insights for the diagnosis, treatment, and prevention of psychiatric disorders. This protocol has been developed and improved over the years by various researchers in Dr. Howland’s laboratory at the University of Saskatchewan.

SARS-CoV-2 has quickly spread all around the globe causing illness and wide damages. Most countries were unprepared for such a rapid spread and crisis. This led to various strategies for effective control of the new pandemic. A key aspect in all countries was to effectively test the population for the virus. Most countries chose a lockdown strategy in which many workplaces and activities are completely closed, leading to substantial economy costs. Here, we present a protocol we recently developed that allows rapid and simple detection of SARS-CoV-2 for the large population, eliminating costs and involvement of professional teams and laboratories. This protocol is based on Reverse Transcribed Loop-Mediated Isothermal Amplification (RT-LAMP). We tested this protocol directly on patient samples, both nasal and throat clinical swabs as well as saliva. Notably, this protocol is simple, cheap and can be easily applied to other pathogens as well.

Endogenous retroviruses (ERV) are transposable retroelements that form ~10% of the murine genome and whose family members are differentially expressed throughout embryogenesis. However, precise regulation of ERV in germ cells remains unclear. To investigate ERV expression in oocytes, we adapted a single-cell mRNA-sequencing library preparation method to generate bulk sequencing libraries from growing oocytes in a time- and cost-efficient manner. Here, we present a modified Smart-seq2 protocol that yields full-length cDNA libraries from purified RNA obtained from low numbers of pooled immature or mature oocytes. Using this method, RNA-sequencing libraries can be generated from any rare or difficult-to-isolate populations for subsequent sequencing and retroelement expression analysis.

Different viruses rely on direct cell-to-cell transmission to propagate infection within the infected host. Measuring this mode of transmission in cultured cells is often complicated by the contribution of cell free viruses to spread, and the difficulty to distinguish between primary infected cells that produce the virus and neighboring cells that are the target of spreading. Here, we present a protocol to quantify cell-to-cell transmission of the model pestivirus bovine viral diarrhea virus that is based on the co-culture of producer cells that are infected with a reporter virus expressing mCherry and target cells that stably express GFP. Spread of cell-free viruses is blocked by the presence of a neutralizing antibody in the cell culture medium, and cell-associated transmission is unequivocally quantified by numbering cells that are positive for both GFP and mCherry using automated analysis of fluorescence microscopy images.

Generation of the epitranscriptome through chemical modifications of protein-coding messenger RNAs (mRNAs) has emerged as a new mechanism of post-transcriptional gene regulation. While most mRNA modifications are methylation events, a single acetylated ribonucleoside has been described in eukaryotes, occurring at the N4-position of cytidine (N4-acetylcytidine or ac4C). Using a combination of antibody-based enrichment of acetylated regions and deep sequencing, we recently reported ac4C as a novel mRNA modification that is catalyzed by the N-acetyltransferase enzyme NAT10. In this protocol, we describe in detail the procedures to identify acetylated mRNA regions transcriptome-wide using acetylated RNA immunoprecipitation and sequencing (acRIP-seq).