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Technology Report ARTICLE

Front. Microbiol., 25 February 2019 | https://doi.org/10.3389/fmicb.2019.00260

Rapid Sequencing of Multiple RNA Viruses in Their Native Form

Thidathip Wongsurawat1†, Piroon Jenjaroenpun1†, Mariah K. Taylor2, Jasper Lee2, Aline Lavado Tolardo3, Jyothi Parvathareddy4, Sangam Kandel1,5, Taylor D. Wadley1, Bualan Kaewnapan6, Niracha Athipanyasilp6, Andrew Skidmore7, Donghoon Chung7, Chutikarn Chaimayo6, Michael Whitt2, Wannee Kantakamalakul6, Ruengpung Sutthent6, Navin Horthongkham6, David W. Ussery1,8, Colleen B. Jonsson2 and Intawat Nookaew1,8*
  • 1Department of Biomedical Informatics, College of Medicine, University of Arkansas for Medical Sciences, Little Rock, AR, United States
  • 2Department of Microbiology, Immunology and Biochemistry, The University of Tennessee Health Science Center, Memphis, TN, United States
  • 3Virology Research Center, Ribeirão Preto Medical School, University of São Paulo, Ribeirão Preto, Brazil
  • 4Regional Biocontainment Laboratory, University of Tennessee Health Science Center, Memphis, TN, United States
  • 5Department of Bioinformatics, University of Arkansas at Little Rock, Little Rock, AR, United States
  • 6Department of Microbiology, Faculty of Medicine Siriraj Hospital, Mahidol University, Bangkok, Thailand
  • 7Department of Microbiology and Immunology, University of Louisville, Louisville, KY, United States
  • 8Department of Physiology and Biophysics, College of Medicine, University of Arkansas for Medical Sciences, Little Rock, AR, United States

Long-read nanopore sequencing by a MinION device offers the unique possibility to directly sequence native RNA. We combined an enzymatic poly-A tailing reaction with the native RNA sequencing to (i) sequence complex population of single-stranded (ss)RNA viruses in parallel, (ii) detect genome, subgenomic mRNA/mRNA simultaneously, (iii) detect a complex transcriptomic architecture without the need for assembly, (iv) enable real-time detection. Using this protocol, positive-ssRNA, negative-ssRNA, with/without a poly(A)-tail, segmented/non-segmented genomes were mixed and sequenced in parallel. Mapping of the generated sequences on the reference genomes showed 100% length recovery with up to 97% identity. This work provides a proof of principle and the validity of this strategy, opening up a wide range of applications to study RNA viruses.

Introduction

Infectious disease epidemics are primarily driven by RNA viruses (Woolhouse et al., 2016; Carrasco-Hernandez et al., 2017) and hence are likely agent of future pandemics (Carrasco-Hernandez et al., 2017). Due to the lack of proofreading in RNA polymerases, RNA viruses are error-prone during genome replication, providing a platform for rapid evolution in new environments and hosts. Currently, genome sequences of many viruses are available and served as a powerful resource for molecular surveillance, pathogen characterization, diagnosis, and antiviral drug discovery (DeFilippis et al., 2003). Still, outbreaks of viral diseases are a never-ending challenge. Short-read sequencing methods to recover RNA viral genomes relies on reverse transcription (RT) of RNA to cDNA which requires primer optimization and amplification. These steps introduce many biases, artifacts and make rapid diagnosis difficult (Marston et al., 2013). Alternatively, real-time sequencing using a pocket-sized MinION device Oxford Nanopore Technologies (ONT) skips these steps and makes rapid detection and characterization of emerging pathogens possible (Hoenen et al., 2016; Kilianski et al., 2016; Faria et al., 2017). A shorter procedure on the MinION by elimination of cDNA synthesis step can be accomplished through direct RNA sequencing (dRNA-seq), designed to directly ligate and sequence only polyadenylated RNA, providing strand-specific information and base modifications of RNA (Garalde et al., 2018; Jenjaroenpun et al., 2018). Independent from the poly(A) enrichment, a sequence-specific 3′-adapter for targeting non-polyadenylated RNA can be designed and has been successfully demonstrated (Garalde et al., 2018) and influenza A virus (Keller et al., 2018). Moreover, target sequence capture/hybridization techniques could be applied before sequencing library preparation to enrich viral genetic materials (Dapprich et al., 2016; Eckert et al., 2016; Karamitros and Magiorkinis, 2018). These methods can reduce background noise from host RNAs. However, designing sequence-specific 3′-adaptor or probing sequence needs a prior knowledge of a nucleotide of the target as prerequisite. Therefore, novel RNA viruses, or coinfections might not be discovered by this approach.

We established a rapid procedure and evaluated the feasibility of MinION for complete sequencing of multiple, single-stranded RNA (ssRNA) viruses in a single reaction to obtain complete genomes. Our approach combines (1) poly(A)-tailing using simple enzymatic reaction, (2) native RNA sequencing by MinION, and (3) real-time analysis aiming to simultaneously detect and characterize multiple RNA viruses. A mix of negative(-) and positive(+) ssRNA viruses, including Mayaro virus (MAYV), Venezuelan equine encephalitis virus (VEEV), Chikungunya virus (CHIKV), Zika virus (ZIKV), vesicular stomatitis Indiana virus (VSV), and Oropouche virus (OROV) were used in this demonstration.

Results

To establish an optimal procedure for real-time native RNA sequencing, we performed three experiments. 1) Sequencing two polyadenylated RNA viruses without RT, suggested by the original protocol, 2) Adding poly(A)-tail to non-polyadenylated RNA phage and ZIKVs using E. coli poly(A) polymerase (EPAP), followed by sequencing, and 3) Applying ribosomal RNA (rRNA) depletion step to host-rRNA contaminated samples, followed by poly(A)-tailing and sequencing. Then, we applied the optimized protocol on a mix of all RNA viruses.

In the first scenario, naturally polyadenylated (+)ssRNA alphaviruses, MAYV and VEEV, genome size approximately 11.5 kb, were used. Extracted RNA (see section “Materials and Methods”) of MAYV and VEEV were pooled at approximately the same concentration (∼350 ng) and used for library preparation of the dRNA-seq protocol, following the manufacturer’s recommendations, except the RT step was skipped (see section “Materials and Methods”). The prepared library then was loaded into ONT flow cell and sequenced. The sequenced reads were mapped on the genomes and analyzed (Table 1), resulting in full genome coverage of the both viruses with 716X and 8184X, for MAYV and VEEV, respectively. We obtained 97% sequence identity by consensus polishing. A high viral/host ratio of 21 was observed because the most abundant RNA species in host, rRNAs, were not captured. By this scenario, multiple viral whole genome sequencing of polyadenylated viruses without RT is possible.

TABLE 1
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Table 1. Three optimization scenario.

The second scenario sought to evaluate the feasibility of using the poly(A)-tailing reaction coupled with dRNA-seq, (+)ssRNA. Bacteriophage MS2 was used first. Five hundred nanograms of 3.57 kb RNA was treated with EPAP using an optimized poly(A)-tailing reaction (see section “Materials and Methods”). Poly(A)-tailed RNA was then used as input for library preparation and sequencing in the same way as described above, resulting in a complete read of the bacteriophage genome (Table 1). We then applied the procedure on ZIKV RNA, non-polyadenylated (+)ssRNA with ∼11 kb length, and obtained long-read. In both scenarios, we observed reduced coverage at the 5′ and a heavy coverage bias towards the 3′, however, we found reads that almost spanned the entire genome (Figure 1B). By poly(A)-tailing reaction, the majority of RNA in ZIKV sample was host RNA that could be captured after EPAP treatment resulted very low virus/host ratio of 0.0014. By this scenario, we obtained a rapid procedure to universally detect ssRNA viruses in real-time. The workflow of poly(A)-tailing plus dRNA-seq was accomplished and summarized in Figure 1A. The host RNA contamination problem was taken into account in the next scenario.

FIGURE 1
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Figure 1. Poly(A)-tailing native RNA-seq protocol. (A) The protocol contains three main steps 1) Poly(A)- tailing reaction using E. coli poly(A) polymerase (EPAP) 2) native RNA-seq by nanopore MinION and 3) real-time analysis to retrieve native RNA sequence. (B) An example of sequencing result (reads) that mapped to the bacteriophage MS2 genome. (C) For detection purpose, this protocol can provide mapped RNA sequences within the first two minutes after sequencing. (D) To obtain whole genome and mRNAs, 2–8 h sequencing could provide more complete information.

In the third scenario, we introduced host rRNA depletion step using a rRNA removal kit, to increase the amount of viral RNA reads. The rRNA depletion was performed before poly(A)-tailing and dRNA-seq. The ZIKV sample was used to evaluate changes in ratio of viral/host RNA. We found that introducing the depletion step resulted in a 160-fold increase in proportion of viral RNA reads/ host reads compared to the non-depleted sequencing. However, we observed high proportion of low-quality sequences compared to non-depleted scenario. We further tested the impact on rRNA depletion step on artificial mixing of 2% of bacteriophage MS2 RNA and 98% of total RNA extracted from mouse cells. The rRNA depletion kit was used for the mixture as described above. Again, the proportion of low quality reads was increased as seen in rRNA-depleted ZIKV sample (Table 1). This problem may be associated with the remained compound from the rRNA depletion process that interfere the dRNA-seq chemistry. Therefore, the depletion step need to be further optimized, we decided not to use the depletion step in our protocol, as it may add complexity and increase the low-quality sequences.

Finally, we applied the established procedure to sequence a pool of six RNA viruses including MAYV, VEEV, CHIKV, ZIKV, VSV, and OROV, which were each purified from supernatant of varying cell lines and RNA was extracted from purified virions (see section “Materials and Methods”). This mixed RNA viruses has diversified genomic property i.e., (+)ssRNA, (-)ssRNA, lack/presence of poly(A)-tail, segmented/non-segmented genomes (Table 2). The RNA input from each sample varied from 16 to 66 ng (215 ng in total) (Table 2). Sequencing on MinION was performed for ∼8 h in total with real-time base calling, enabling data analysis in real-time (see section “Materials and Methods”). The sequences were mapped to the viral genomes and host genomes (Table 2). Remarkably, within the first two minutes, the first reads of all six viruses were translocated through nanopore (Figure 1C). In only two hours, complete or near complete genomes of all the six viruses were acquired (Figure 1D). In total 85,711 reads were generated, 5,000 (6%) were mapped on viruses, 62,060 (72%) were mapped on host genomes, and 18,651 (22%) were unclassified (low quality). Mapping of the 5,000 reads on the six genomes showed 100% recovery of the MAYV, VEEV, CHIKV, VSV, and OROV at 48X – 659X coverage and showed 99% recovery of the ZIKV, the least abundance in the mix, at 10X coverage (Table 2). We obtained several long reads (>10 kb) that covered > 95% of MAYV, VEEV, and VSV genomes while the longest reads mapped to CHIKV and ZIKV were 84 and 68% of genome length, respectively. Unlike the other viruses, OROV has a tripartite genome of small (S), medium (M), and large (L) segments. We found the longest read covered 99% of S (0.96 kb), 98% of M and L (4.39 kb and 6.85 kb). Notably, although high error rates of individual native RNA sequence were observed (∼82% read identity), 93–97% identity can be achieved by consensus polishing.

TABLE 2
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Table 2. List of virus used in this study and sequencing result.

We inspected the mapped reads based on strand-orientation and found feasibility of simultaneous detection of viral genome and its transcripts (Figure 2). We observed the two spikes of read coverage depth around the gap of two subgenomic mRNA of VEEV on the coverage plot (Figure 2A) clearly indicating that the two subgenomic mRNAs were independently transcribed and the reads that spanned over the gap belonged to the genomic material (see section “Materials and Methods”). This result is based on sequencing RNA directly without primer bias, RT and amplification. However, observation of two subgenomic mRNA in VEEV need further deep investigation. Conversely, (-)ssRNA virus needs to transcribe mRNA in the opposite direction of the genome. We found mapped reads derived from the mRNA and genome of OROV nicely aligned in opposite direction (Figure 2B).

FIGURE 2
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Figure 2. Strand-specific sequencing of (+)/(-)ssRNA. (A) Mapped sequences (coverage depth) of (+)ssRNA genome venezuelan equine encephalitis virus and subgenomic RNA were plotted in the same direction as shown integrative genomics viewer (IGV). The top panel shows all mapped reads. The middle panel shows the three categories of mapped reads belong to genome (gRNA) and the two subgenomic mRNA(sgRNA). The bottom panel shows the zoom in view of non-subgenomic mRNA region that enable discrimination between genome and subgenomic RNA (B) Mapped sequences (coverage depth) of (-) ssRNA Oropouche virus genome (gRNA) and mRNA were plotted in the opposite direction. Black: positive strand and Gray: negative strand. At the 5′end to corner of each coverage plot shows scale of sequencing depth. The dark gray boxes in the bottom of each panel were gene annotation. Top, middle and bottom panel illustrated the three segment S, M, and L of OROV, respectively. The details of mismatches and the general quality of the reads mapping for panel (A,B) are visualize in Supplementary Figure S1.

Discussion

This versatile protocol can contribute viral RNA research by (i) retaining the strand direction; this facilitates simultaneously detection of genome, subgenomic mRNA/mRNA, recombinant, complementary RNA intermediates (ii) increasing the accuracy of determining transcriptomic architecture and recombination with no need for assembly (iii) providing a fast and easy method to perform direct sequencing of any RNA virus (iv) directly sequencing of novel RNA viruses with no specific primer required, including novel ones and (v) saving on the budget (see Table 3). In addition, the native RNA signal can be used for further detection of RNA base modifications (RNA epigenetics) that are known to control viral replication during host infection (Lichinchi et al., 2016). The RNA base modifications, occurred on native RNA sequence, alter the ionic current signal recorded during dRNA-seq (Garalde et al., 2018), leading to the errors on the sequence that is not stochastic (Wongsurawat et al., 2018). By comparison the error of native RNA sequence with its complementary DNA (cDNA) sequence, which contains no error from base modification after RT, multiple RNA modification types can be captured (Wongsurawat et al., 2018). The ability to generate multiple levels of genetic information at high speed has potential to increase our basic understanding of the known and undiscovered viruses at a rapid rate. Although promising, however, this protocol carries a number of limitations. First, this protocol requires high amounts of virus. The dRNA-seq detection limit in respect of viral copy number need to be further investigated for clinical application. Second, the poly(A)-tail reaction is not only specific to viral RNA; host RNA can also be a target. Competition between host RNAs and viral genome requires a better strategy for host RNAs depletion. Third, although we could identify virus at species-level from error-prone long reads, deep sequencing is required for accurate strain-level identification. However, improvement of nanopore read accuracy is subject to extensive research, and it is likely that much better accuracy will be available in the future, as well as better depth of viral reads, leading to strain-level identification. In conclusion, our simple protocol could provide rapid viral RNA genome/subgenome sequencing and characterization that can be therefore a versatile tool to study biology of RNA viruses.

TABLE 3
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Table 3. Advantages and limitations of this protocol.

Materials and Methods

Viral Cultivation and RNA Extraction

Mayaro Virus (MAYV), Oropouche Virus (OROV), and Venezuelan Equine Encephalitis Virus (VEEV)

Mayaro virus (strain BeAr505411, Genbank No: KP842818.1), OROV (strain BeAn 19991, Genbank No: S: KP052852.1; Segment M: KP052851.1; Segment L: KP052850.1) and VEEV (strain TC-83, Genbank no: L01443.1) were cultivated on Vero cells in MEM with 5%FBS and 1%PenStrep. The infection was made on 80% confluent cells with an MOI of 1 for MAYO and 0.5 for OROV. Both viruses were incubated with cells for 3 days. The viruses were then aliquoted and centrifuged according to protocol. The TRIzol LS extraction (Invitrogen) was carried out following the manufacturer’s instruction for RNA extraction with the exception of adding glycogen after separating the aqueous phase from the organic layer and interphase. Purified RNA was resuspended in 50 μl RNase-free water and stored at -70°C.

Chikungunya Virus (CHIKV)

CHIKV (strain 181/25 was obtained from BEI resources, Genbank no: EF452493.1) was propagated in Vero 76 cells (ATCC CRL-1587) grown in MEM-E with 10% FBS. After CPE was monitored, the cell supernatant was harvested and clarified with a low-speed centrifugation at 4,000 ×g for 20 min. The cell supernatant was stored at -80°C until use and viral RNA was isolated from the supernatants. RNA was isolated using RNAzol RT (MRC) with the Direct-zol RNA miniprep kit (Zymo Research) according to manufacturer’s instructions, with one additional wash step.

Vesicular Stomatitis Indiana Virus (VSV)

BHK-21 cells were infected at a multiplicity of 0.1 and the culture medium was collected after 22 h. The culture media were first clarified by centrifuging at 8,000 ×g for 10 min then the supernatants were layered on top of a 20% sucrose cushion and pelleted at 100,000 ×g for 1 h. The virus pellet was resuspended in Tris–saline, pH 7.4 and stored at -80°C. The viral pellet was subjected to a phenol-chloroform RNA extraction from TRIzol LS (Invitrogen) following manufacturer’s protocol with the exception of adding glycogen after separating the aqueous phase from the organic layer and interphase. Purified RNA was resuspended in 20 μl RNase-free water and stored at -70°C.

Zika Virus (ZIKV)

Two strains of ZIKV were used for this study.

(1) Genomic RNA of ZIKV (strain MR 766, GenBank: AY632535.2) used for method optimization was purchased from ATCC.1

(2) ZIKV (strain PRVABC59 provided by Dr. Barbara Johnson at CDC, GenBank: KU501215) used in pooled viruses sequencing was propagated in Vero 76 cells grown in MEME (GIBCO Laboratories) with 10% fetal bovine serum. After CPE was monitored, the cell supernatant was harvested and clarified with a low-speed centrifugation at 4,000 × g for 20 min. The cell supernatant was stored at -80°C until use and viral RNA was isolated from the supernatants. RNA was isolated using RNAzol RT (MRC) with the Direct-zol RNA miniprep kit (Zymo Research) according to manufacturer’s instructions, with one additional wash step.

Bacteriophage MS2 RNA

RNA from bacteriophage MS2 (Sigma) is composed of 3569 nucleotides (Genbank no: NC_001417.2). MS2 RNA is free of host nucleic acids and proteins.2

Mouse RNA

RNA isolation was performed from a mouse cell line with the Direct-Zol RNA miniprep Kit (Zymo Research) as per manufacturer’s instructions. Total RNA was eluted in 50 μl nuclease free water and stored at -80°C.

Ribosomal RNA (rRNA) Depletion

Host cytoplasmic and mitochondrial rRNA was depleted from the samples using Ribo-Zero Gold kit (Illumina) according to manufacturer’s instructions. Briefly, magnetic beads were washed, samples were treated with rRNA removal solution, rRNA was removed, and rRNA-depleted samples were purified.

RNA Quantification

RNA was quantified using a Qubit® 2.0 Fluorometer (ThermoFisher Scientific) and Nanodrop Spectrophotometer (ThermoFisher Scientific). The Qubit® assay uses a Qubit RNA BR (Broad-Range) Assay Kit (ThermoFisher Scientific).

Poly(A)-Tailing of RNA Using E. coli Poly(A) Polymerase (EPAP)

To obtain high quality RNA for further preparation, extracted RNA of each virus received from a different independent lab was purified and concentrated using AMPureXP beads (Beckman Coulter) and eluted in 15 μl nuclease-free water (NEB). Purified and concentrated RNA was incubated at 70°C for 2 min and immediately placed on ice to avoid secondary structure formation. Poly(A)-tailing reaction using E. coli EPAP (NEB# M0276) was designed to perform in a 26 μl reaction (reaction size can be scaled up as needed). Purified RNA was treated with 2.5 μl 10X E. coli Poly(A) Polymerase Reaction Buffer (supplied with the enzyme), 4.5 μl ATP (10 mM) (supplied with the enzyme), and 4 μl EPAP (NEB) at 37°C for 10 min. Poly(A)-tailed RNA was then cleaned using 2.5× (by volume) AMPureXP beads (Beckman Coulter) and eluted with 11–15 μl nuclease free water (NEB), 2 min at room temperature. Cleaned Poly(A)-tailed RNA was incubated for 1 min at 70°C and immediately placed on ice to remove secondary structure. The cleaned Poly(A)-tailed RNA was used as input for dRNA-seq library preparation.

Library Preparation and Direct RNA Sequencing by Nanopore

Direct RNA sequencing was performed using the Direct RNA Sequencing Protocol (SQK-RNA001 kit) for the MinION. Some steps of the manufacture protocol were modified. First, the ligation reaction of RNA and adaptor was extended from 10 to 15 min. At this step, control RNA (RCS) was not added. Second, the RT (50 min) step was skipped in our protocol. Third, wire-bored tips (Axygen) were used for mixing AMPureXP beads (Beckman Coulter)-RNA. RNA library was eluted and loaded onto a flow cell for sequencing. Sequencing of the RNA was performed on a single R9.4/FLO-MIN106 flow cell on a MinION Mk1B for ∼8 h.

Bioinformatics and Real-Time Analysis

Immediately after loading the library onto a flow cell and sequencing, base-calling was started using the local-based software, Albacore version 2.3.1 (ONT) with the (–disable_filtering -q 0) command modifications from default. We first filtered out the sequenced reads below a size of 200 bases to avoid short, low-quality reads. The remaining reads were mapped to viral genomes and the host genomes using Minimap2 version 2.9 (Li, 2018) with the -k 7 from virus and -k 14 for host command modifications from default. The aligned reads were processed in downstream analysis. The number of mapped reads in virus and hosts were measured by Samtools version 1.5 (Li et al., 2009). The read coverage was calculated using genomecov package in BEDtools version 2.27.1 (Quinlan and Hall, 2010) and visualized using IGV (Robinson et al., 2011). The reference-based assembly was performed using four rounds consensus polishing of the reference genomes by Racon version 1.2.1 (Vaser et al., 2017).

Data Availability

The sequence native RNA data of six viruses has been submitted to GenBank and is publicly available under the Bioproject number PRJNA493665.

Author Contributions

IN and TW designed and conceived the project. IN, CJ, and DU supervised the study. CJ, MT, JL, AT, JP, BK, NA, AS, DC, CC, MW, WK, RS, and NH performed viral cultivation and RNA extraction. TDW and TW optimized library preparation protocol. TW and SK conducted MinION sequencing. PJ and IN performed computational analysis. All authors participated in interpreting the results and writing the manuscript, and read and approved the final version of this manuscript.

Funding

This work was funded in part by the Helen Adams & Arkansas Research Alliance Endowed Chair, the National Institute of General Medical Sciences of the National Institutes of Health award no. P20GM125503 and National Institutes of Health award no R01AI103053.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2019.00260/full#supplementary-material.

Footnotes

  1. ^ https://www.atcc.org/products/all/VR-84.aspx
  2. ^ https://www.sigmaaldrich.com/catalog/product/roche/10165948001?lang=en\&region=US

References

Carrasco-Hernandez, R., Jacome, R., Lopez Vidal, Y., and Ponce de Leon, S. (2017). Are RNA viruses candidate agents for the next global pandemic? A review. ILAR J. 58, 343–358. doi: 10.1093/ilar/ilx026

PubMed Abstract | CrossRef Full Text | Google Scholar

Dapprich, J., Ferriola, D., Mackiewicz, K., Clark, P. M., Rappaport, E., D’Arcy, M., et al. (2016). The next generation of target capture technologies - large DNA fragment enrichment and sequencing determines regional genomic variation of high complexity. BMC Genomics 17:486. doi: 10.1186/s12864-016-2836-6

PubMed Abstract | CrossRef Full Text | Google Scholar

DeFilippis, V., Raggo, C., Moses, A., and Fruh, K. (2003). Functional genomics in virology and antiviral drug discovery. Trends Biotechnol. 21, 452–457. doi: 10.1016/S0167-7799(03)00207-5

CrossRef Full Text | Google Scholar

Eckert, S. E., Chan, J. Z., Houniet, D., PATHSEEK consortium, Breuer, J., and Speight, G. (2016). Enrichment by hybridisation of long DNA fragments for Nanopore sequencing. Microb. Genom 2:e000087. doi: 10.1099/mgen.0.000087

PubMed Abstract | CrossRef Full Text | Google Scholar

Faria, N. R., Quick, J., Claro, I. M., Theze, J., de Jesus, J. G., Giovanetti, M., et al. (2017). Establishment and cryptic transmission of Zika virus in Brazil and the Americas. Nature 546, 406–410. doi: 10.1038/nature22401

PubMed Abstract | CrossRef Full Text | Google Scholar

Garalde, D. R., Snell, E. A., Jachimowicz, D., Sipos, B., Lloyd, J. H., Bruce, M., et al. (2018). Highly parallel direct RNA sequencing on an array of nanopores. Nat. Methods 15, 201–206. doi: 10.1038/nmeth.4577

PubMed Abstract | CrossRef Full Text | Google Scholar

Hoenen, T., Groseth, A., Rosenke, K., Fischer, R. J., Hoenen, A., Judson, S. D., et al. (2016). Nanopore sequencing as a rapidly deployable ebola outbreak tool. Emerg. Infect. Dis. 22, 331–334. doi: 10.3201/eid2202.151796

PubMed Abstract | CrossRef Full Text | Google Scholar

Jenjaroenpun, P., Wongsurawat, T., Pereira, R., Patumcharoenpol, P., Ussery, D. W., Nielsen, J., et al. (2018). Complete genomic and transcriptional landscape analysis using third-generation sequencing: a case study of Saccharomyces cerevisiae CEN.PK113-7D. Nucleic Acids Res. 4:e38. doi: 10.1093/nar/gky014

PubMed Abstract | CrossRef Full Text | Google Scholar

Karamitros, T., and Magiorkinis, G. (2018). Multiplexed targeted sequencing for oxford nanopore MinION: a detailed library preparation procedure. Methods Mol. Biol. 1712, 43–51. doi: 10.1007/978-1-4939-7514-3_4

PubMed Abstract | CrossRef Full Text | Google Scholar

Keller, M. W., Rambo-Martin, B. L., Wilson, M. M., Ridenour, C. A., Shepard, S. S., Stark, T. J., et al. (2018). Direct RNA sequencing of the coding complete influenza A virus genome. Sci. Rep. 8:14408. doi: 10.1038/s41598-018-32615-8

PubMed Abstract | CrossRef Full Text | Google Scholar

Kilianski, A., Roth, P. A., Liem, A. T., Hill, J. M., Willis, K. L., Rossmaier, R. D., et al. (2016). Use of unamplified RNA/cDNA-hybrid nanopore sequencing for rapid detection and characterization of RNA viruses. Emerg. Infect. Dis. 22, 1448–1451. doi: 10.3201/eid2208.160270

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, H. (2018). Minimap2: pairwise alignment for nucleotide sequences. Bioinformatics 34, 3094–3100. doi: 10.1093/bioinformatics/bty191

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, H., Handsaker, B., Wysoker, A., Fennell, T., Ruan, J., Homer, N., et al. (2009). The Sequence Alignment/Map format and SAMtools. Bioinformatics 25, 2078–2079. doi: 10.1093/bioinformatics/btp352

PubMed Abstract | CrossRef Full Text | Google Scholar

Lichinchi, G., Zhao, B. S., Wu, Y., Lu, Z., Qin, Y., He, C., et al. (2016). Dynamics of human and viral RNA methylation during Zika Virus infection. Cell Host. Microbe 20, 666–673. doi: 10.1016/j.chom.2016.10.002

PubMed Abstract | CrossRef Full Text | Google Scholar

Marston, D. A., McElhinney, L. M., Ellis, R. J., Horton, D. L., Wise, E. L., Leech, S. L., et al. (2013). Next generation sequencing of viral RNA genomes. BMC Genomics 14:444. doi: 10.1186/1471-2164-14-444

PubMed Abstract | CrossRef Full Text | Google Scholar

Quinlan, A. R., and Hall, I. M. (2010). BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics 26, 841–842. doi: 10.1093/bioinformatics/btq033

PubMed Abstract | CrossRef Full Text | Google Scholar

Robinson, J. T., Thorvaldsdottir, H., Winckler, W., Guttman, M., Lander, E. S., Getz, G., et al. (2011). Integrative genomics viewer. Nat. Biotechnol. 29, 24–26. doi: 10.1038/nbt.1754

PubMed Abstract | CrossRef Full Text | Google Scholar

Vaser, R., Sovic, I., Nagarajan, N., and Sikic, M. (2017). Fast and accurate de novo genome assembly from long uncorrected reads. Genome Res. 27, 737–746. doi: 10.1101/gr.214270.116

PubMed Abstract | CrossRef Full Text | Google Scholar

Wongsurawat, T., Jenjaroenpun, P., Wassenaar, T. M., Wadley, T. D., Wanchai, V., Akel, N. N., et al. (2018). Decoding the epitranscriptional landscape from native RNA sequences. bioRXiv [Preprint]. doi: 10.1101/487819

CrossRef Full Text | Google Scholar

Woolhouse, M. E., Brierley, L., McCaffery, C., and Lycett, S. (2016). Assessing the epidemic potential of RNA and DNA viruses. Emerg. Infect. Dis. 22, 2037–2044. doi: 10.3201/eid2212.160123

PubMed Abstract | CrossRef Full Text | Google Scholar

Keywords: native RNA, genome, subgenomic mRNA, single-stranded RNA, virus, nanopore sequencing, rapid detection, MinION

Citation: Wongsurawat T, Jenjaroenpun P, Taylor MK, Lee J, Tolardo AL, Parvathareddy J, Kandel S, Wadley TD, Kaewnapan B, Athipanyasilp N, Skidmore A, Chung D, Chaimayo C, Whitt M, Kantakamalakul W, Sutthent R, Horthongkham N, Ussery DW, Jonsson CB and Nookaew I (2019) Rapid Sequencing of Multiple RNA Viruses in Their Native Form. Front. Microbiol. 10:260. doi: 10.3389/fmicb.2019.00260

Received: 18 November 2018; Accepted: 31 January 2019;
Published: 25 February 2019.

Edited by:

Sead Sabanadzovic, Mississippi State University, United States

Reviewed by:

Timokratis Karamitros, University of Oxford, United Kingdom
Pasquale Saldarelli, Institute for Sustainable Plant Protection (IPSP-CNR), Italy

Copyright © 2019 Wongsurawat, Jenjaroenpun, Taylor, Lee, Tolardo, Parvathareddy, Kandel, Wadley, Kaewnapan, Athipanyasilp, Skidmore, Chung, Chaimayo, Whitt, Kantakamalakul, Sutthent, Horthongkham, Ussery, Jonsson and Nookaew. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Intawat Nookaew, inookaew@uams.edu

These authors have contributed equally to this work