Mini Review ARTICLE
The Role of HCMV and HIV-1 MicroRNAs: Processing, and Mechanisms of Action during Viral Infection
- 1Immuno-Oncology Laboratory, Oncohaematology Department, Bambino Gesù Children’s Hospital, Istituto di Ricovero e Cura a Carattere Scientifico, Rome, Italy
- 2Angiogenesis Laboratory, Oncohaematology Department, Bambino Gesù Children’s Hospital, Istituto di Ricovero e Cura a Carattere Scientifico, Rome, Italy
- 3RNA Editing Laboratory, Oncohaematology Department, Bambino Gesù Children’s Hospital, Istituto di Ricovero e Cura a Carattere Scientifico, Rome, Italy
Viruses infect host cells releasing their genome (DNA or RNA) containing all information needed to replicate themselves. The viral genome takes control of the cells and helps the virus to evade the host immune system. Some viruses alter the functions of infected cells without killing them. In some cases infected cells lose control over normal cell proliferation and becomes cancerous. Viruses, such as HCMV and HIV-1, may leave their viral genome in the host cells for a certain period (latency) and begin to replicate when the cells are stressed causing diseases. HCMV and HIV-1 have developed multiple strategies to avoid recognition and elimination by the host’s immune system. These strategies rely on viral products that mimic specific components of the host cells to prevent immune recognition of virally infected cells. In addition to viral proteins, viruses encode short non-coding RNAs (vmiRNAs) that regulate both viral and host cellular transcripts to favor viral infection and actively curtail the host’s antiviral immune response. In this review, we will give an overview of the general functions of microRNAs generated by HCMV and HIV-1, their processing and interaction with the host’s immune system.
MicroRNAs (miRNAs) are short (∼22 nucleotides) single-stranded non-coding RNA molecules that negatively regulate gene expression at post-transcriptional level. The miRNA maturation machinery involves several steps and multiple proteins in both nucleus and cytoplasm. miRNAs can be transcribed as part of independent primary transcripts (pri-miRNAs), which are mainly generated by RNA polymerase II (Lee et al., 2004; Ozsolak et al., 2008), and display all features commonly associated with Pol II-mediated transcription, such as histone marks, CpG islands, transcription factor binding sites (Cai et al., 2004). In the canonical miRNA biogenesis pathway, the Microprocessor complex, a multiprotein complex with Drosha and Di George Syndrome critical region gene 8 (DGCR8), cleaves the double-stranded pri-miRNA generating a hairpin-shaped RNA molecule (pre-miRNA) of about 70–100 bp (Denli et al., 2004; Han et al., 2006). This process can be modulated by different proteins (Suzuki et al., 2009; Trabucchi et al., 2009). Once generated, nuclear pre-miRNAs are exported to the cytoplasm by the exportin-5/Ran-GTP complex to be further processed by the RNase III enzyme Dicer (Grishok et al., 2001). The pre-miRNA processing is finely regulated and its inhibition affects miRNA-mediated differentiation in embryonic stem cells, embryonal carcinoma cells and certain primary tumors. An example is provided by Lin-28, an developing regulated RNA binding protein, which promotes cell proliferation and tumorigenesis of embryonic cells by affecting let-7 maturation (Viswanathan et al., 2008). The activity of Dicer can be either enhancing or inhibiting by A-to-I RNA editing mediated by ADARs enzymes which convert Adenosine to Inosine (Kawahara et al., 2008; Nishikura, 2010; Tomaselli et al., 2013). ADAR1 has been shown to directly bind Dicer, thus increasing the maximum rate of pre-microRNA cleavage by Dicer (Ota et al., 2013). In human adult brain, it has been estimated that approximately 20% of pri-miRNAs can undergo A-to-I RNA editing (Nishikura, 2010; Tomaselli et al., 2013) by affecting miRNAs maturation at different steps (Luciano et al., 2004; Chawla and Sokol, 2014; Tomaselli et al., 2015).
The result of Dicer cleavage is the formation of a double stranded RNA of 22 nt in length whose strand with the less stability is normally chosen as guide strand and transferred to the RNA-induced silencing complex (RISC) for the annealing of miRNAs to the target mRNA, whereas the other strand [the star (∗)-strand] is usually degraded. The RISC complex contains Dicer and many associated proteins such as Argonaute (Ago) protein family and the RNA-binding protein TRBP [human immunodeficiency virus transactivating response RNA (TAR) binding protein] (Chendrimada et al., 2005).
Mature miRNAs recognize their target mRNAs through 6–8 nucleotides (the seed region) at the 5′ end of the miRNA. Complete complementarity between the miRNA and target mRNA sequence directs mRNA degradation, while absent of perfect complementarity will silence the gene target by preventing its translation (Lim et al., 2005). A given miRNA may have hundreds of different mRNA targets, and a given target mRNA might be regulated by several miRNAs. These evidences suggest that the biogenesis of miRNAs is extremely complex and regulated at different levels, thus highlighting the importance of these short RNA molecules in crucial cell programs including viral infection.
Viruses have developed multiple strategies to avoid recognition and elimination by the host’s immune system. These strategies rely on viral products that mimic specific components of the host cells to prevent immune recognition of virally infected cells. In addition to viral proteins, viruses encode miRNAs (vmiRNA) that regulate both viral and host cellular transcripts during viral infection. The first vmiRNAs was identified in a cell line latently infected with Epstein–Barr virus (EBV) (Pfeffer et al., 2004), a member of the Herpesviridae, that in humans is associated with Burkitt’s lymphoma, Hodgkin’s disease and nasopharyngeal carcinoma (Raab-Traub, 2007). Currently, different members of Herpesviridae, Polyomaviridae and Adenoviridae families are known to express vmiRNAs (Skalsky and Cullen, 2010). To date, 172 viral-encoded mature miRNAs are listed in the miRBase collection1 (Kozomara and Griffiths-Jones, 2014), the majority of which (93%) belongs to the three subfamilies (Alphaherpesvirinae, Betaherpesvirinae and Gammaherpesvirinae) of Herpesviridae family (Figure 1).
Biogenesis of vmiRNAs largely relies on host-derived machineries. The common pathway of vmiRNA maturation involves the transcription from host RNA polymerase II into a long transcript precursor known as viral pri-miRNA (vpri-miRNAs), which is trimmed by the host RNase III endonuclease Drosha microprocessor into approximately 80 nt long hairpin structures, known as viral pre-miRNAs (vpre-miRNAs). Vpre-miRNAs are rapidly exported to the cytoplasm where a specialized multi-domain ribonuclease III enzyme, known as Dicer, removes the loop structure leaving the vmiRNA duplex. Some functional vmiRNAs, such as murine γ-herpesvirus 68 (MHV68) miRNAs, are produced by host RNA polymerase III and tRNase Z, independently from the microprocessor-Drosha component (Bogerd et al., 2010), whereas others are generated by different additional non-canonical pathways (Pfeffer et al., 2005; Diebel et al., 2010, 2014; Kincaid et al., 2012; Burke et al., 2014; Feldman et al., 2014; Kincaid et al., 2014; Whisnant et al., 2014).
In general, virus and the host-cell’s miRNAs use different mechanisms to interfere each other. Viruses can either block or impair the host cells miRNA pathway by interacting with key proteins (Lu and Cullen, 2004; Bennasser et al., 2006), synthesize and regulate their own miRNAs (Grundhoff and Sullivan, 2011; Harwig et al., 2014), exploit cellular miRNAs to complete their replication cycle (Luna et al., 2015). Conversely, host cells can target vmiRNAs with endogenous miRNAs (Lecellier et al., 2005; Delorme-Axford et al., 2013; Bai and Nicot, 2015). The complex interplay between viruses and host cells usually favors viral infection by either reducing immune recognition or promoting cell growth and lytic or latent infection. One of the best examples of virus-host-miRNA interplay important for human infection and diseases come from HCMV. In this review, we summarize the general functions of miRNAs generated by HCMV and their interactions with immune system and we discuss new finding regarding miRNA from HIV-1.
HCMV is a ubiquitous and highly specific herpesvirus that establishes lifelong latent infections, coexisting asymptomatically with its host in a healthy immune system, with periodic and spontaneous phases of reactivation, lytic replication and virus shedding (Stern-Ginossar et al., 2012). In immunocompromised individuals, such as transplant recipients, HIV-infected patients and individuals with an immunological immaturity, as the fetus in utero, HCMV can cause different clinical syndromes the severity of which depends on the degree of immunosuppression (Varani and Landini, 2011). Of note, during pregnancy HCMV primary infections can lead to mental retardation and severe neonatal pathologies.
To persist indefinitely within the host, HCMV has elaborated several strategies that act to subvert host cellular immune responses (Noriega et al., 2012). Many HCMV proteins and vmiRNAs are known to target cellular and viral transcripts to establish and maintain latency (Murphy et al., 2008). The complex interplay between virus and host is further enhanced by post-transcriptional events, such as RNA editing. Indeed, during HCMV infection, the expression of the short form of the RNA editing enzyme ADAR1 (ADAR1-p110) is enhanced and the host miR-376a precursor undergo editing at specific sites. The increased edited-miR-376a during HCMV infection, downregulates HLA-E transcript leading the infected cells more visible by NK cells (Nachmani et al., 2014).
To date, 15 stem-loop precursors and 26 mature HCMV miRNAs are deposited in the miRBase (Figure 2). HCMV miRNAs are differently expressed during latent and lytic infection. Of note, only a subset of vmiRNAs are produced during HCMV latency, most of which originate from the unique long (UL) region of the HCMV genome (Meshesha et al., 2016). Interestingly, during reactivation of the virus from latency all known vmiRNAs, including those that were absent during latency, restored their expression. An alternative expression of the two stands of miR-US29 was detected in the lytic and latent infection. Specifically, miR-US29-5p prevailed during lytic infection, whereas miR-US29-3p dominated viral latency, suggesting the presence of a specific mechanism that regulates expression of the two arms of the vmiRNA hairpins during the viral life cycle (Meshesha et al., 2016). It is possible that expression of vmiRNAs during latency is required to manipulate host-signaling pathways and make the latently infected cell ready for reactivation.
FIGURE 2. Genomic organization of the miRNAs encoded by HCMV and HIV-1. Location of precursors (red) and mature (black) miRNAs is shown by hairpin loop structures along the linear representation of the HCMV (A) and HIV-1 (B) genomes. miRNAs shown above the line representing viral double-strand DNA are transcribed in sense direction (from right to left), while those shown below are transcribed in the opposite direction.
HCMV miRNAs are known to target several cellular genes to evade immune system, control cell cycle and vesicle trafficking (Table 1). Since this subject has been recently reviewed by Piedade and Azevedo-Pereira (2016), in this review we will deepen the HCMV miRNAs with proved implications in viral evasion from innate and adaptive immune responses.
The first host cellular mRNA target reported for a HCMV vmiRNA encodes MICB, a stress-induced ligand for the NK cell activating receptor NKG2D critical for the NK cell killing of virus-infected and tumor cells. VmiR-UL112 specifically binds to MICB-3′ untranslated regions (3′UTR) and downregulates MICB expression during viral infection, therefore, leading to decreased binding of NKG2D and reduced killing by NK cells (Stern-Ginossar et al., 2007). This miRNA-mediated MICB inhibition is not exclusive to HCMV, but conserved in the herpesviruses family. Other viral miRNAs encoded by EBV and HHV-8 (miR-BART2-5p and miR-k12-7, respectively), target MICB to escape NK cell recognition (Nachmani et al., 2009). These vmiRNAs exhibit poor sequence homology with HCMV miR-UL112 and target MICB at different binding sites. HCMV miR-UL112 attenuates NK cell activity also by targeting others transcripts, such as IL-32, type I IFN and the toll-like receptor 2 (TLR2) signaling (Landais et al., 2015).
In addition, the HCMV miR-UL148D, one of the most highly expressed vmiRNAs during latent infection, contribute to immune evasion by directly targeting the chemokine (C-C Motif) ligand 5 (CCL5), a chemokine known to attract immune cells to sites of inflammation and tissue damage (Kim et al., 2012). This downregulation was reverted by treatment with a miR-UL148D-specific inhibitor, supporting the role of this agent as therapeutic tool against HCMV infection. VmiR-UL148D also targets the activating receptor type-1B (ACVR1B) in monocytes, resulting in a reduced secretion of IL-6 (Lau et al., 2016). More recently, vmiR-US5-1 and vmiR-UL112-3p have been shown to play important role in modulating NF-κB signaling at late time of infection by reducing the expression of the IKK complex and induce the release of proinflammatory cytokines (Hancock et al., 2017). The limited or delayed secretion of proinflammatory cytokines is thought to be one of the mechanisms of immune evasion exploited by vmiRNAs to limit the recruitment of immune cells and killing of infected cells.
Finally, the HCMV miR-US4-1 was shown to directly target the endoplasmic reticulum aminopeptidase 1 (ERAP1), a key peptidase that trims peptide precursors to their optimal length to bind MHC class I molecules (Kim et al., 2011). The reduced trimming due to HCMV-specific action resulted in an immuno-evasion of HCMV-infected cells (Kim et al., 2011).
All these mechanisms focus on the possibility to enhance viral replication by hindering viral clearance by NK cells and T cells for the period of time necessary to virus to replicate.
HIV-1 infection cause progressive CD4+ T-cell loss making individuals susceptible to get infections and develop a wide range of immunological abnormalities until oncological complications. Although HIV infections are able to induce vigorous antiviral immune responses, HIV-1 replication is not fully controlled by the innate and adaptive immune system. Like many other viruses, HIV-1 has evolved a number of strategies to evade host immune responses, most notably by using viral accessory proteins and RNA.
Recent reports have demonstrated the existence of HIV-1-derived miRNAs from coding and non-coding regions of the viral genome, which regulate both viral and host gene expression (Table 1). Despite so, the presence of HIV-1 derived vmiRNAs has been highly controversial and further studies are necessary to better understand their potential role in viral infection and pathogenesis. The importance of viral and cell host miRNAs in the context of HIV-1 infection was first suggested by silencing of Drosha and Dicer leading to significant enhancement of HIV-1 replication (Triboulet et al., 2007). The first description of HIV-1-derived miRNAs came in 2004 from a group that identified a Nef-derived miRNA, named miR-N367 (Omoto et al., 2004). MiR-N367 reduces HIV-1 transcription by blocking Nef expression and long terminal repeat (LTR) transcription (Omoto et al., 2004; Omoto and Fujii, 2005). The HIV-1 transactivation RNA (TAR), which regulates viral translation, also encodes for a vmiRNA (called TAR-miR-5p and -3p) (Ouellet et al., 2008; Klase et al., 2009). TAR-miR has been shown to downregulate host genes (such as ERCC1 and IER3) important for apoptosis and cell survival, thus giving HIV-1-infected cells a survival advantage by preventing host cell death (Klase et al., 2009). Recent studies demonstrated that additional host substrates, including Caspase 8, Aiolos, Ikaros and Nucleophosmin (NPM)/B23, are modulated by TAR-miR (Ouellet et al., 2013). VmiR-H1, located in the LTR has been reported to downregulate the apoptosis-antagonizing transcription factor (AATF) gene product and act as an antagonist of the anti-apoptotic effect mediated by TAR-miR. Additionally, hiv1-mir-H1 can downregulate the host miR149 expression recognized to target HIV-1 Vpr transcript (Kaul et al., 2009). Recently, Zhang et al. (2014) have reported the existence of a novel HIV-1-encoded vmiRNA called miR-H3 located in the region of the HIV-1 RNA genome that encodes for reverse transcriptase (RT). Overexpression of miR-H3 increases viral production and mutations within miR-H3 sequence significantly impair the viral replication of wild-type HIV-1 viruses by targeting HIV-1 5′-LTR (TATA box) (Zhang et al., 2014). Two additional vmiRNAs (called as vmiR88 and vmiR99) were identified in overlapping regions of HIV LTR from viral infected human macrophages (Bernard et al., 2014). They were able to directly stimulate TNFα release by human macrophages through TLR8 activation by a mechanism that is partially dependent on vmiRNA sequence motifs. Of note, vmiR88 and vmiR99 were detected in sera of HIV infected individuals suggesting their role in stimulating recipient macrophages in vivo and contributing to chronic immune activation.
Future Outlook and Conclusion
vmiRNAs have overall a protecting role for the viral infection. By interfering with host cellular proteins and mechanisms of immune evasion, they represent a potential target for future specific therapies. Studies on the complex interplay between viral miRNAs and host genes has been only recently started and further investigations are required to identify more efficient and less toxic therapeutic strategies. The identification of differentially expressed miRNAs during viral infection (for example in HIV-1 infection) may provide a new approach to control disease progression. Finally, understanding the mechanism of vmiRNA-mediated immune evasion will allow us to develop novel strategies to prevent and cure viral infections. Targeting vmiRNAs with molecules such as antagomirs may represent a novel therapeutic strategy to limit chronic immune activation and the progression of viral infection.
DF and AG analyzed the literature, wrote the manuscript, and approved the final version for publication. RR analyzed the literature, revised the manuscript and approved the final version for publication.
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.
This work was supported by Italian Ministry of Health (Rome, Italy) grant PE-2011-02351866 (DF) and Associazione Italiana per la Ricerca sul Cancro (AIRC, Milan, Italy) grants # 18495 (DF), # 17615 (AG) and # 15312 (RR).
Bai, X. T., and Nicot, C. (2015). miR-28-3p is a cellular restriction factor that inhibits human T cell leukemia virus, type 1 (HTLV-1) replication and virus infection. J. Biol. Chem. 290, 5381–5390. doi: 10.1074/jbc.M114.626325
Bennasser, Y., Yeung, M. L., and Jeang, K. T. (2006). HIV-1 TAR RNA subverts RNA interference in transfected cells through sequestration of TAR RNA-binding protein, TRBP. J. Biol. Chem. 281, 27674–27678. doi: 10.1074/jbc.C600072200
Bernard, M. A., Zhao, H., Yue, S. C., Anandaiah, A., Koziel, H., and Tachado, S. D. (2014). Novel HIV-1 miRNAs stimulate TNFalpha release in human macrophages via TLR8 signaling pathway. PLoS ONE 9:e106006. doi: 10.1371/journal.pone.0106006
Bogerd, H. P., Karnowski, H. W., Cai, X., Shin, J., Pohlers, M., and Cullen, B. R. (2010). A mammalian herpesvirus uses noncanonical expression and processing mechanisms to generate viral microRNAs. Mol. Cell. 37, 135–142. doi: 10.1016/j.molcel.2009.12.016
Burke, J. M., Bass, C. R., Kincaid, R. P., and Sullivan, C. S. (2014). Identification of tri-phosphatase activity in the biogenesis of retroviral microRNAs and RNAP III-generated shRNAs. Nucleic Acids Res. 42, 13949–13962. doi: 10.1093/nar/gku1247
Chendrimada, T. P., Gregory, R. I., Kumaraswamy, E., Norman, J., Cooch, N., Nishikura, K., et al. (2005). TRBP recruits the Dicer complex to Ago2 for microRNA processing and gene silencing. Nature 436, 740–744. doi: 10.1038/nature03868
Delorme-Axford, E., Donker, R. B., Mouillet, J. F., Chu, T., Bayer, A., Ouyang, Y., et al. (2013). Human placental trophoblasts confer viral resistance to recipient cells. Proc. Natl. Acad. Sci. U.S.A. 110, 12048–12053. doi: 10.1073/pnas.1304718110
Diebel, K. W., Claypool, D. J., and Van Dyk, L. F. (2014). A conserved RNA polymerase III promoter required for gammaherpesvirus TMER transcription and microRNA processing. Gene 544, 8–18. doi: 10.1016/j.gene.2014.04.026
Fan, J., Zhang, W., and Liu, Q. (2014). Human cytomegalovirus-encoded miR-US25-1 aggravates the oxidised low density lipoprotein-induced apoptosis of endothelial cells. Biomed. Res. Int. 2014:531979. doi: 10.1155/2014/531979
Feldman, E. R., Kara, M., Coleman, C. B., Grau, K. R., Oko, L. M., Krueger, B. J., et al. (2014). Virus-encoded microRNAs facilitate gammaherpesvirus latency and pathogenesis in vivo. MBio 5:e981-14. doi: 10.1128/mBio.00981-14
Grey, F., Meyers, H., White, E. A., Spector, D. H., and Nelson, J. (2007). A human cytomegalovirus-encoded microRNA regulates expression of multiple viral genes involved in replication. PLoS Pathog. 3:e163. doi: 10.1371/journal.ppat.0030163
Grey, F., Tirabassi, R., Meyers, H., Wu, G., Mcweeney, S., Hook, L., et al. (2010). A viral microRNA down-regulates multiple cell cycle genes through mRNA 5’UTRs. PLoS Pathog. 6:e1000967. doi: 10.1371/journal.ppat.1000967
Grishok, A., Pasquinelli, A. E., Conte, D., Li, N., Parrish, S., Ha, I., et al. (2001). Genes and mechanisms related to RNA interference regulate expression of the small temporal RNAs that control C. elegans developmental timing. Cell 106, 23–34. doi: 10.1016/S0092-8674(01)00431-7
Guo, X., Huang, Y., Qi, Y., Liu, Z., Ma, Y., Shao, Y., et al. (2015). Human cytomegalovirus miR-UL36-5p inhibits apoptosis via downregulation of adenine nucleotide translocator 3 in cultured cells. Arch. Virol. 160, 2483–2490. doi: 10.1007/s00705-015-2498-8
Han, J., Lee, Y., Yeom, K. H., Nam, J. W., Heo, I., Rhee, J. K., et al. (2006). Molecular basis for the recognition of primary microRNAs by the Drosha-DGCR8 complex. Cell 125, 887–901. doi: 10.1016/j.cell.2006.03.043
Hancock, M. H., Hook, L. M., Mitchell, J., and Nelson, J. A. (2017). Human cytomegalovirus microRNAs miR-US5-1 and miR-UL112-3p block proinflammatory cytokine production in response to NF-kappaB-activating factors through direct downregulation of IKKalpha and IKKbeta. mBio 8:e00109-17. doi: 10.1128/mBio.00109-17
Hook, L. M., Grey, F., Grabski, R., Tirabassi, R., Doyle, T., Hancock, M., et al. (2014). Cytomegalovirus miRNAs target secretory pathway genes to facilitate formation of the virion assembly compartment and reduce cytokine secretion. Cell Host Microbe 15, 363–373. doi: 10.1016/j.chom.2014.02.004
Huang, Y., Chen, D., He, J., Cai, J., Shen, K., Liu, X., et al. (2015). Hcmv-miR-UL112 attenuates NK cell activity by inhibition type I interferon secretion. Immunol. Lett. 163, 151–156. doi: 10.1016/j.imlet.2014.12.003
Huang, Y., Qi, Y., Ma, Y., He, R., Ji, Y., Sun, Z., et al. (2013). The expression of interleukin-32 is activated by human cytomegalovirus infection and down regulated by hcmv-miR-UL112-1. Virol. J. 10:51. doi: 10.1186/1743-422X-10-51
Kawahara, Y., Megraw, M., Kreider, E., Iizasa, H., Valente, L., Hatzigeorgiou, A. G., et al. (2008). Frequency and fate of microRNA editing in human brain. Nucleic Acids Res. 36, 5270–5280. doi: 10.1093/nar/gkn479
Kim, S., Lee, S., Shin, J., Kim, Y., Evnouchidou, I., Kim, D., et al. (2011). Human cytomegalovirus microRNA miR-US4-1 inhibits CD8(+) T cell responses by targeting the aminopeptidase ERAP1. Nat. Immunol. 12, 984–991. doi: 10.1038/ni.2097
Kim, Y., Lee, S., Kim, S., Kim, D., Ahn, J. H., and Ahn, K. (2012). Human cytomegalovirus clinical strain-specific microRNA miR-UL148D targets the human chemokine RANTES during infection. PLoS Pathog. 8:e1002577. doi: 10.1371/journal.ppat.1002577
Kincaid, R. P., Chen, Y., Cox, J. E., Rethwilm, A., and Sullivan, C. S. (2014). Noncanonical microRNA (miRNA) biogenesis gives rise to retroviral mimics of lymphoproliferative and immunosuppressive host miRNAs. MBio 5:e00074-14. doi: 10.1128/mBio.00074-14
Klase, Z., Winograd, R., Davis, J., Carpio, L., Hildreth, R., Heydarian, M., et al. (2009). HIV-1 TAR miRNA protects against apoptosis by altering cellular gene expression. Retrovirology 6:18. doi: 10.1186/1742-4690-6-18
Landais, I., Pelton, C., Streblow, D., Defilippis, V., Mcweeney, S., and Nelson, J. A. (2015). Human cytomegalovirus miR-UL112-3p targets TLR2 and modulates the TLR2/IRAK1/NFkappaB signaling pathway. PLoS Pathog. 11:e1004881. doi: 10.1371/journal.ppat.1004881
Lau, B., Poole, E., Krishna, B., Sellart, I., Wills, M. R., Murphy, E., et al. (2016). The expression of human cytomegalovirus microRNA MiR-UL148D during latent infection in primary myeloid cells inhibits activin A-triggered secretion of IL-6. Sci. Rep. 6:31205. doi: 10.1038/srep31205
Lecellier, C. H., Dunoyer, P., Arar, K., Lehmann-Che, J., Eyquem, S., Himber, C., et al. (2005). A cellular microRNA mediates antiviral defense in human cells. Science 308, 557–560. doi: 10.1126/science.1108784
Lim, L. P., Lau, N. C., Garrett-Engele, P., Grimson, A., Schelter, J. M., Castle, J., et al. (2005). Microarray analysis shows that some microRNAs downregulate large numbers of target mRNAs. Nature 433, 769–773. doi: 10.1038/nature03315
Murphy, E., Vanicek, J., Robins, H., Shenk, T., and Levine, A. J. (2008). Suppression of immediate-early viral gene expression by herpesvirus-coded microRNAs: implications for latency. Proc. Natl. Acad. Sci. U.S.A. 105, 5453–5458. doi: 10.1073/pnas.0711910105
Nachmani, D., Stern-Ginossar, N., Sarid, R., and Mandelboim, O. (2009). Diverse herpesvirus microRNAs target the stress-induced immune ligand MICB to escape recognition by natural killer cells. Cell Host Microbe 5, 376–385. doi: 10.1016/j.chom.2009.03.003
Nachmani, D., Zimmermann, A., Oiknine Djian, E., Weisblum, Y., Livneh, Y., Khanh Le, V. T., et al. (2014). MicroRNA editing facilitates immune elimination of HCMV infected cells. PLoS Pathog. 10:e1003963. doi: 10.1371/journal.ppat.1003963
Ota, H., Sakurai, M., Gupta, R., Valente, L., Wulff, B. E., Ariyoshi, K., et al. (2013). ADAR1 forms a complex with Dicer to promote microRNA processing and RNA-induced gene silencing. Cell 153, 575–589. doi: 10.1016/j.cell.2013.03.024
Ouellet, D. L., Plante, I., Landry, P., Barat, C., Janelle, M. E., Flamand, L., et al. (2008). Identification of functional microRNAs released through asymmetrical processing of HIV-1 TAR element. Nucleic Acids Res. 36, 2353–2365. doi: 10.1093/nar/gkn076
Ouellet, D. L., Vigneault-Edwards, J., Letourneau, K., Gobeil, L. A., Plante, I., Burnett, J. C., et al. (2013). Regulation of host gene expression by HIV-1 TAR microRNAs. Retrovirology 10:86. doi: 10.1186/1742-4690-10-86
Pan, C., Zhu, D., Wang, Y., Li, L., Li, D., Liu, F., et al. (2016). Human cytomegalovirus miR-UL148D facilitates latent viral infection by targeting host cell immediate early response gene 5. PLoS Pathog. 12:e1006007. doi: 10.1371/journal.ppat.1006007
Pfeffer, S., Sewer, A., Lagos-Quintana, M., Sheridan, R., Sander, C., Grasser, F. A., et al. (2005). Identification of microRNAs of the herpesvirus family. Nat. Methods 2, 269–276. doi: 10.1038/nmeth746
Qi, M., Qi, Y., Ma, Y., He, R., Ji, Y., Sun, Z., et al. (2013). Over-expression of human cytomegalovirus miR-US25-2-3p downregulates eIF4A1 and inhibits HCMV replication. FEBS Lett. 587, 2266–2271. doi: 10.1016/j.febslet.2013.05.057
Raab-Traub, N. (2007). “EBV-induced oncogenesis,” in Human Herpesviruses: Biology, Therapy, and Immunoprophylaxis, eds A. Arvin, G. Campadelli-Fiume, E. Mocarski, P. S. Moore, B. Roizman, R. Whitley, et al. (Cambridge: Cambridge University Press).
Shao, Y., Qi, Y., Huang, Y., Liu, Z., Ma, Y., Guo, X., et al. (2016). Human cytomegalovirus-encoded miR-US4-1 promotes cell apoptosis and benefits discharge of infectious virus particles by targeting QARS. J. Biosci. 41, 183–192. doi: 10.1007/s12038-016-9605-1
Stern-Ginossar, N., Elefant, N., Zimmermann, A., Wolf, D. G., Saleh, N., Biton, M., et al. (2007). Host immune system gene targeting by a viral miRNA. Science 317, 376–381. doi: 10.1126/science.1140956
Tirabassi, R., Hook, L., Landais, I., Grey, F., Meyers, H., Hewitt, H., et al. (2011). Human cytomegalovirus US7 is regulated synergistically by two virally encoded microRNAs and by two distinct mechanisms. J. Virol. 85, 11938–11944. doi: 10.1128/JVI.05443-11
Tomaselli, S., Bonamassa, B., Alisi, A., Nobili, V., Locatelli, F., and Gallo, A. (2013). ADAR enzyme and miRNA story: a nucleotide that can make the difference. Int. J. Mol. Sci. 14, 22796–22816. doi: 10.3390/ijms141122796
Tomaselli, S., Galeano, F., Alon, S., Raho, S., Galardi, S., Polito, V. A., et al. (2015). Modulation of microRNA editing, expression and processing by ADAR2 deaminase in glioblastoma. Genome Biol. 16:5. doi: 10.1186/s13059-014-0575-z
Trabucchi, M., Briata, P., Garcia-Mayoral, M., Haase, A. D., Filipowicz, W., Ramos, A., et al. (2009). The RNA-binding protein KSRP promotes the biogenesis of a subset of microRNAs. Nature 459, 1010–1014. doi: 10.1038/nature08025
Triboulet, R., Mari, B., Lin, Y. L., Chable-Bessia, C., Bennasser, Y., Lebrigand, K., et al. (2007). Suppression of microRNA-silencing pathway by HIV-1 during virus replication. Science 315, 1579–1582. doi: 10.1126/science.1136319
Wang, Y. P., Qi, Y., Huang, Y. J., Qi, M. L., Ma, Y. P., He, R., et al. (2013). Identification of immediate early gene X-1 as a cellular target gene of hcmv-mir-UL148D. Int. J. Mol. Med. 31, 959–966. doi: 10.3892/ijmm.2013.1271
Whisnant, A. W., Kehl, T., Bao, Q., Materniak, M., Kuzmak, J., Lochelt, M., et al. (2014). Identification of novel, highly expressed retroviral microRNAs in cells infected by bovine foamy virus. J. Virol. 88, 4679–4686. doi: 10.1128/JVI.03587-13
Keywords: microRNA, HCMV, HIV, immune system, cancer
Citation: Fruci D, Rota R and Gallo A (2017) The Role of HCMV and HIV-1 MicroRNAs: Processing, and Mechanisms of Action during Viral Infection. Front. Microbiol. 8:689. doi: 10.3389/fmicb.2017.00689
Received: 17 December 2016; Accepted: 04 April 2017;
Published: 21 April 2017.
Edited by:Francisco J. Enguita, Universidade de Lisboa, Portugal
Reviewed by:Dmitri Sviridov, Baker IDI Heart and Diabetes Institute, Australia
George Calin, University of Texas MD Anderson Cancer Center, USA
Copyright © 2017 Fruci, Rota and Gallo. 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) or licensor 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.