Abstract
Cytomegalovirus (CMV) is a pathogen that is common worldwide and is often present in individuals infected with human immunodeficiency virus (HIV). Pattern recognition receptors (PRRs) are host sensors that activate the immune response against infectious agents. However, it is unclear whether PRR single-nucleotide polymorphisms (SNPs) are associated with the occurrence of CMV DNAemia in subjects coinfected with HIV and CMV. HIV/CMV-coinfected patients with and without CMV DNAemia were recruited for this study. The DDX58 rs10813831 and IFIH1 (rs3747517 and rs1990760) polymorphisms were genotyped using the TaqMan Allelic Discrimination Assay, whereas the DDX58 rs12006123 and TLR3 (rs3775291 and rs3775296) SNPs were analyzed using a polymerase chain reaction restriction fragment length polymorphism (PCR-RFLP) assay. A mutation present in at least one allele of the DDX58 rs12006123 SNP occurred at least two times more frequently in HIV/CMV-coinfected patients with CMV DNAemia than in coinfected subjects without CMV DNAemia (OR, 2.50; 95% CI, 1.33–4.68; p = 0.004, in the dominant model). A higher level of CMV DNAemia was observed in subjects who had the heterozygous (GA) or homozygous recessive (AA) genotype for the DDX58 rs12006123 SNP compared with those who had the wild-type (GG) genotype (p = 0.0003). Moreover, in subjects with a mutation detected in at least one allele of the DDX58 rs12006123 SNP, a lower serum IFN-β concentration was found compared with those who had a wild-type (GG) genotype for this polymorphism (p = 0.024). The DDX58 rs12006123 SNP is associated with CMV DNAemia in HIV/CMV-coinfected patients.
Similar content being viewed by others
Avoid common mistakes on your manuscript.
Introduction
Human immunodeficiency virus (HIV), a member of the genus Lentivirus, family Retroviridae, is one of the most common bloodborne pathogens and one of the most devastating human diseases of the 21st century. In HIV-infected individuals, coinfection with cytomegalovirus (CMV; genus Cytomegalovirus, family Orthoherpesviridae) contributes to increased systemic inflammation, chronic immune activation, and immunosenescence, despite effective antiretroviral therapy (ART) [1, 2]. In HIV-positive patients who are stable on ART, the associations between levels of CMV antibodies, cardiovascular risk, and neurocognitive health are moderated by age-associated increases in the response to CMV, while an independent link between CMV antibodies and insulin resistance has been observed [3]. Additionally, active CMV replication is common in HIV-infected individuals [4, 5] and is associated with low CD4+/CD8+ ratios [1, 5].
During viral infections, pattern recognition receptors (PRRs), including endosomal Toll-like receptors (TLRs) and cytoplasmic RNA helicases such as retinoic acid-inducible gene (RIG)-I-like receptors (RLRs) initiate antiviral immunity via induction of type I and III interferons (IFNs) as well as inflammatory cytokines. These receptors are expressed in various tissues and cell types, including dendritic cells, neutrophils, macrophages, lymphocytes, and epithelial cells [6, 7]. It has been reported that the homozygous recessive (TT) genotype of the TLR3 rs3775291 single-nucleotide polymorphism (SNP) provided resistance to HIV infection in Spanish HIV-exposed seronegative (HESN) intravenous drug users (IDUs), and individuals with this genotype sustained lower levels of viral replication [8]. In another study, a mutation present in at least one allele of this SNP was also associated with protection against HIV infection in Estonian HESN IDUs [9]. An association between CT and TT genotypes of the TLR9 2848C/T SNP and the occurrence of CMV DNAemia in HIV/CMV-coinfected patients has also been described [4]. Here, we report a correlation between DDX58 rs12006123 SNP and CMV DNAemia in HIV/CMV-coinfected patients.
The aim of this investigation was to assess whether polymorphisms in the TLR3 and RLR genes (DDX58, encoding RIG-I and IFIH1, encoding MDA5) have an impact on the occurrence of CMV DNAemia in HIV-infected patients with a CMV-seropositive status. The association between these SNPs and the concentrations of selected cytokines was also studied.
Materials and methods
Participants
Whole peripheral blood and serum samples were collected from 192 HIV/CMV-coinfected adults (median age, 37.7; range, 17–72 years) recruited from the Department of Infectious Diseases and Hepatology, Medical University of Lodz (Lodz, Poland). Subjects were consecutively enrolled from November 2006 to August 2008 and from May 2017 to March 2018. Patients with positive tests for HIV and CMV antibodies were included in the study. All HIV-infected patients received combined ART (e.g., tenofovir [TDF or TAF]/emtricitabine [FTC], abacavir [ABC]/lamivudine [3TC] combined with an integrase or protease inhibitor or a nonnucleoside reverse transcriptase inhibitor). HIV quantification was performed using the Cobas AmpliPrep/Cobas TaqMan HIV-1 test, v2.0 (Roche Diagnostics GmbH, Mannheim, Germany) on a Light Cycler 480 thermal cycler (Roche Diagnostics GmbH). CMV infection was diagnosed by the detection of CMV DNA in whole blood of patients with specific anti-CMV IgG antibodies present in their serum samples. CMV IgG was measured using LIAISON assay (DiaSorin, Saluggia, Italy) according to the manufacturer’s recommendations. CMV DNAemia was quantified in all participants after study entry at a median of 4.9 years after initiation of ART (range, 0.3–21.4 years; Table 1). All participants included in the study were of Caucasian origin and were recruited from the same geographical region. This study was performed in accordance with the Helsinki Declaration and with good clinical practice guidelines and was approved by the appropriate ethics committees (RNN/211/06/KE and RNN/33/17/KE). All volunteers gave written informed consent to donate samples for research purposes.
Analysis of RLR and TLR SNPs
Genomic DNA was isolated from peripheral blood using a QIAamp DNA Blood Mini Kit (QIAGEN GmbH, Hilden, Germany) according to the manufacturer’s recommendations. The DDX58 rs10813831 (C_1552406_10), IFIH1 rs3747517 (C_25984418_10), and IFIH1 rs1990760 (C_2780299_30) SNPs were genotyped using a TaqMan Allelic Discrimination Assay (Applied Biosystems, Carlsbad, CA, USA) and TaqMan Genotyping Master Mix (Thermo Fisher Scientific, Vilnius, Lithuania) using a 7900HT Fast Real-Time PCR system (Applied Biosystems, Foster City, CA, USA). SNP genotyping was performed using 10 ng of genomic DNA, 1.25 µl of TaqMan Allelic Discrimination Assay Mix, and 12.50 µl of TaqMan Genotyping Master Mix in a final volume of 25 µl. The initial denaturation step was performed at 95°C for 10 min, followed by 40 cycles of denaturation at 95°C for 15 s and annealing at 60°C for 60 s. Genotyping for the DDX58 rs12006123 and TLR3 (rs3775291 and rs3775296) SNPs was performed using a polymerase chain reaction restriction fragment length polymorphism (PCR-RFLP) assay as described elsewhere [10, 11]. In brief, PCR products were digested with the restriction enzyme SsiI (AciI), HpyF3I, or MboII (Fermentas, Hanover, MD, USA), and the digested fragments were separated using a QIAxcel capillary electrophoresis system (QIAGEN GmbH, Hilden, Germany). Randomly selected samples of each PRR SNP were confirmed using a 96-capillary 3730xl DNA Analyzer (Applied Biosystems).
Assessment of CMV DNAemia
CMV DNAemia was defined as the presence of detectable CMV DNA in the patient’s blood samples. The CMV DNA copy number was determined using a 7900HT Fast Real-Time PCR System (Applied Biosystems) as described previously [12]. The amplification was performed using a primer set recognizing sequences within the UL55 gene (gB1, GAG GAC AAC GAA ATC CTG TTG GGC A; gB2, GTC GAC GGT GGA GAT ACT GCT GAG G; TaqMan probe, CAA TCA TGC GTT TGA AGA GGT AGT CCA) [12]. Briefly, PCR assays were carried out in a final volume of 25 µl containing 5 µl of patient DNA, 12.5 µl of TaqMan Universal PCR Master Mix (Applied Biosystems), 0.1 µl of the primer set (100 pmol/µl), 0.05 µl of probe (100 pmol/µl) labeled with FAM (6-carboxyfluoroscein) and TAMRA (6-carboxytetramethylrhodamine), and 7.25 µl of deionized water. DNA samples were amplified as follows: preincubation at 95°C for 10 min, followed by 50 cycles of 15 s at 95°C and 60 s at 60°C. To validate the assay, a negative control without template DNA was included in each amplification run. The analytical sensitivity of the assay was determined to be 2 × 102 copies/ml. The UL55 gene was cloned using a TOPO Kit for Sequencing, with One Shot TOP10 Chemically Competent E. coli (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s instructions. The resulting clones were sequenced in both directions to confirm that no point mutations had been introduced during the amplification process. High-quality plasmid DNA was purified using a PureLink Quick Plasmid Miniprep Kit (Invitrogen) according to the manufacturer’s recommendations.
Measurement of cytokine levels
Cytokine levels were measured using a BD Cytometric Bead Array (CBA) Human Th1/Th2/Th17 Cytokine Kit (BD Biosciences, San Jose, CA, USA). This assay simultaneously measures the concentration of IL-2, IL-4, IL-6, IL-10, IL-17A, TNF, and IFN-γ. Serum samples were measured on an LSR II BD flow cytometer (BD Biosciences, Franklin Lakes, NJ, USA) and analyzed using FCAP Array software (BD Biosciences). Levels of IFN-α, IFN-β (PBL Assay Science, Piscataway, NJ, USA), and IL-7 (Thermo Scientific, Frederick, MD, USA) were determined using ELISA kits according to the manufacturer’s instructions.
Statistical analysis
Statistical analysis was performed using GraphPad Prism version 5.0 (GraphPad Software, San Diego, CA, USA) or SPSS 25.0 for Windows (SPSS Inc., Chicago, Illinois, USA). Baseline data were expressed as the median and range for nonnormal continuous variables or numbers (percentages) for categorical variables. Experimental data were analyzed using nonparametric Fisher’s exact test, the chi-square test, or the Mann-Whitney U test, when appropriate. Differences were regarded as statistically significant when the p-value was ≤ 0.05. Hardy-Weinberg equilibrium (HWE), linkage disequilibrium (LD), and haplotype analyses were performed using SNPStats software (http://www.snpstats.net/start.htm). The p-values were corrected for multiple tests with a Bonferroni correction; the significance level for pB was 0.010 instead of the standard 0.05 (raw p-value/5).
Results
Clinical characteristics of patients
Of the 192 HIV/CMV-coinfected patients tested using a commercial polymerase chain reaction (PCR) assay, 161 (83.9%) had undetectable levels of HIV RNA. The CMV IgG antibodies were detected in all patients with HIV/CMV coinfection. Forty-one subjects had a CD4+ T cell count ≤ 200 cells/mm3 (including 28 patients with CMV DNAemia and 13 subjects without CMV DNAemia), and 151 had a CD4+ T cell count > 200 cells/mm3 (including 80 patients with CMV DNAemia and 71 subjects without CMV DNAemia; Table 1).
The heterozygous genotype of the TLR3 rs3775291 SNP is prevalent in patients with CMV DNAemia
First, the DDX58 rs10813831, rs12006123; IFIH1 rs1990760, rs3747517; and TLR3 rs3775291 and rs3775296 SNPs were genotyped in 192 HIV/CMV-coinfected patients. The DDX58 rs12006123 GG genotype and the TLR3 rs3775296 CC genotype were detected less frequently in HIV/CMV-coinfected patients with CMV DNAemia than in subjects without CMV DNAemia (22.2% vs. 41.7%, p = 0.004, and 28.7% vs. 46.4%, p = 0.011, respectively). The heterozygous (CT) genotype of the TLR3 rs3775291 polymorphism was more common in HIV/CMV-coinfected patients with CMV DNAemia than in those without CMV DNAemia (56.5% vs. 39.3%, p = 0.018). No significant differences were found for the DDX58 rs10813831 and IFIH1 rs1990760 and rs3747517 SNPs. Interestingly, the homozygous recessive (AA) genotype of the DDX58 rs12006123 SNP was observed more frequently in HIV/CMV-coinfected patients with CD4+ T counts below 200 cells/mm3 than in those with CD4+ T counts > 200 cells/mm3 (OR, 4.60; 95% CI, 1.61–13.13; p = 0.013). A higher prevalence of low CD4+ T-cell counts (CD4+ T-cell count ≤ 200 cells/mm3) in HIV/CMV-coinfected patients with a heterozygous (GA) or homozygous recessive (AA) genotype of the DDX58 rs10813831 polymorphism (OR, 2.62; 95% CI, 1.27–5.40; p = 0.007) was also noted. The observed genotype and allele frequencies of the TLR3 rs3775296 SNP were not in HWE (p > 0.05) and were excluded from further analysis.
The DDX58 rs12006123 SNP is frequent in HIV/CMV-coinfected patients with CMV DNAemia
The heterozygous (GA) and homozygous recessive (AA) genotypes of DDX58 rs12006123 occurred more frequently in HIV/CMV-coinfected patients with CMV DNAemia than in coinfected subjects without CMV DNAemia (OR, 2.50; 95% CI, 1.33–4.68; p = 0.004, in the dominant model; Table 2). This SNP showed a higher rate of occurrence of CMV DNAemia even after Bonferroni correction for multiple tests (pB = 0.010). The heterozygous (CT) genotype of the TLR3 rs3775291 SNP was detected more commonly in HIV/CMV-coinfected patients with CMV DNAemia than in those without CMV DNAemia (OR, 2.01; 95% CI, 1.12–3.58; p = 0.018, in the overdominant model). However, this finding did not reach statistical significance after Bonferroni correction for multiple tests (pB > 0.010).
PRR SNPs are associated with CMV DNAemia
Of the 192 HIV/CMV-coinfected patients, 56.3% had detectable levels of CMV DNA in their peripheral blood. A higher level of CMV viremia was observed in patients who were heterozygous (GA) or homozygous recessive (AA) for the DDX58 rs12006123 SNP (median, 1.31 × 102 copies/ml; range, 0-3.22 × 106 copies/ml) than in those who had a wild-type (GG) genotype for this polymorphism (median, 9.40 × 102 copies/ml; range, 0-1.02 × 104 copies/ml; p = 0.0003). The median CMV DNAemia was also higher among subjects who were homozygous recessive (TT) for the TLR3 rs3775291 SNP (median, 2.78 × 102 copies/ml; range, 0-3.22 × 106 copies/ml) compared with those who were heterozygous (CT) or had a wild-type (CC) genotype for this polymorphism (median, 1.36 × 102 copies/ml; range, 0-9.34 × 105 copies/ml; p = 0.047). No other associations were found (p > 0.05).
Haplotype analysis
Haplotype analysis of DDX58 rs10813831, rs12006123; IFIH1 rs1990760, rs3747517; and TLR3 rs3775291 SNPs revealed two haploblocks: DDX58 and IFIH1. The haplotype GA of the DDX58 haploblock was detected in 37.0% of HIV/CMV-coinfected patients with CMV DNAemia and in 25.5% of coinfected subjects without CMV DNAemia and was associated with a twofold increased incidence of CMV DNAemia (OR, 2.10; 95% CI, 1.21–3.37; p = 0.010). For the IFIH1 haploblock, the most prevalent haplotype was CC (59.3% of cases); however, no association with the incidence of CMV DNAemia in HIV/CMV-coinfected patients was noted. A tight LD was found for the adjacent SNPs in the coding region of IFIH1 rs3747517 and rs1990760 (r2 = 0.45).
Association of PRR SNPs with cytokine production
To investigate the clinical relevance of PRR SNPs and the outcome of coinfection, the serum concentrations of 10 target cytokines in the examined patients were measured (Table 1). The levels of IL-2, IL-17A, and IFN-γ were below the standard range in all patients. In subjects with a mutation detected in at least one allele of the DDX58 rs12006123 SNP, a lower serum IFN-β concentration was found compared with those who had a wild-type (GG)
genotype for this polymorphism (median, 0 pg/ml; range, 0-2935 pg/ml vs. median, 209.7
pg/ml; range, 0-574.7 pg/ml; p = 0.024). Individuals with a wild-type (CC) genotype for the TLR3 rs3775291 SNP had a higher serum IFN-β concentration than those who were heterozygous (CT) or homozygous recessive (TT) for this polymorphism (median, 0 pg/ml; range, 0-2935 pg/ml vs. median, 0 pg/ml; range, 0-2922 pg/ml; p = 0.026). Moreover, the serum IL-7 concentration was lower in HIV/CMV-coinfected patients with the TLR3 rs3775291 CC and CT genotypes compared with patients with the TT genotype (median, 37.3 pg/ml; range, 0-1100.0 pg/ml vs. median, 55.0 pg/ml; range, 4.4-825.1 pg/ml; p = 0.041). No other cytokines showed associations with PRR SNPs.
Discussion
To our knowledge, this is the first study to assess the relationship between TLR3 and RLR gene polymorphisms and the occurrence of CMV DNAemia in HIV/CMV-coinfected adults. The DDX58 rs12006123 and TLR3 rs3775291 SNPs were associated with a higher incidence of CMV DNAemia among HIV/CMV-coinfected patients as well as with higher DNA CMV loads in the peripheral blood. Mutations present in at least one allele of these polymorphisms were associated with a lower serum IFN-β concentration, and a link between the CD4+ T cell count and PRR SNPs was noted.
HIV-1, a member of the family Retroviridae, is one of the most intriguing and challenging viruses of the last century. The present study revealed that the DDX58 rs12006123 and the TLR3 rs3775291 SNPs are associated with a higher incidence of CMV DNAemia in HIV/CMV-coinfected patients and with higher DNA CMV loads. It was reported recently that the TLR3 rs3775291 CT genotype was associated with the early stage of HIV infection among individuals naïve to ART, with a higher frequency in the advanced stage of HIV infection compared to healthy subjects [13]. Interestingly, the heterozygous (GA) genotypes of the DDX58 rs12006123 and rs10813831 SNPs were more frequently observed in HIV/CMV-coinfected individuals with CD4+ T counts below 200 cells/mm3. It is well known that the persistence of latent HIV proviruses in CD4+ T cells, despite combined ART, is a major roadblock to HIV eradication. It was found recently that stimulation of the RIG-I pathway enhanced RIG-I signaling ex vivo, increased HIV transcription, and induced apoptosis of HIV-infected CD4+ T cells [14]. Other studies, however, showed that RIG-I-dependent IFN activation was not significant and was insufficient to induce the death of latently infected HIV-positive cells [15, 16]. We therefore hypothesize that cells carrying DDX58 polymorphisms might act as a cellular reservoir of HIV that takes advantage of the immune environment to facilitate HIV persistence and replication.
PRRs are a family of germline-encoded receptors that play a pivotal role in the host’s early response to invading pathogens and subsequent adaptive immunity. TLR3 and RIG-I recognize double-stranded RNA (dsRNA), produced during viral replication or release from apoptotic cells [15, 17, 18], and activate specific signaling pathways that lead to induction of type I and III IFN and/or production of inflammatory cytokines. However, the mechanism by which DDX58 rs12006123 polymorphisms regulate the host response against HIV/CMV coinfection remains unclear. The DDX58 rs12006123 SNP is located in the 3’UTR region of the RIG-I gene and does not lead to an amino acid change. It was reported that the DDX58 rs12006123 SNP did not affect allele-specific mRNA expression in human dendritic cells [11]. However, one study has shown a significant reduction in measles-virus-induced IFN-γ and IL-2 secretion in peripheral blood mononuclear cells of measles-virus-infected patients with the DDX58 rs12006123 SNP [19].
In the present study, the TLR3 rs3775291 CC and CT genotypes were associated with a lower serum IL-7 concentration. IL-7 is known to be essential for de novo T cell generation in the thymus, and it contributes to the maintenance of peripheral T cell homeostasis. It has been shown that the CD4+ and CD8+ T cell populations downregulate the IL-7 receptor in response to IL-7 and other pro-survival cytokines (e.g., IL-2, IL-4, IL-6, and IL-15), and IL-7 also contributes to T cell development, homeostatic proliferation, and survival [20, 21]. Recently, clinical trials have shown that repeated cycles of recombinant IL-7 injections are safe and could improve the immune response by affecting CD4+ T cell proliferation and survival [22, 23]. It is therefore plausible that a cellular mechanism (e.g., immune reconstitution inflammatory syndrome) or other SNPs in linkage disequilibrium can have a direct effect on the individual SNP.
There are some potential limitations to this study. First, this work was conducted on a small number of HIV/CMV-coinfected volunteers. Second, all HIV/CMV-coinfected subjects received combined ART therapy, which can modulate the immune response. Therefore, larger studies are necessary in the future to confirm the association between PRR polymorphisms and CMV DNAemia in HIV-infected subjects.
Overall, this study showed that the DDX58 rs12006123 polymorphism might be associated with a higher incidence of CMV DNAemia in HIV/CMV-coinfected adults. An effect of PRR polymorphisms on cytokine concentrations was also observed. The results suggest a broad area for further studies of the dynamic nature of the intermolecular interactions between pathogens and host receptors.
Data availability
The current study has no associated data.
References
Caby F, Guihot A, Lambert-Niclot S, Guiguet M, Boutolleau D, Agher R, Valantin MA, Tubiana R, Calvez V, Marcelin AG, Carcelain G, Autran B, Costagliola D, Katlama C (2016) Determinants of a Low CD4/CD8 Ratio in HIV-1-Infected Individuals Despite Long-term Viral Suppression. Clin Infect Dis 62:1297–1303. https://doi.org/10.1093/cid/ciw076
Lichtner M, Cicconi P, Vita S, Cozzi-Lepri A, Galli M, Lo Caputo S, Saracino A, De Luca A, Moioli M, Maggiolo F, Marchetti G, Vullo V, d’Arminio Monforte A, ICONA Foundation Study (2015) Cytomegalovirus coinfection is associated with an increased risk of severe non-AIDS-defining events in a large cohort of HIV-infected patients. J Infect Dis 211:178–186. https://doi.org/10.1093/infdis/jiu417
Brunt SJ, Cysique LA, Lee S, Burrows S, Brew BJ, Price P (2016) Short Communication: Do Cytomegalovirus Antibody Levels Associate with Age-Related Syndromes in HIV Patients Stable on Antiretroviral Therapy? AIDS Res Hum Retroviruses 32:567–572. https://doi.org/10.1089/AID.2015.0328
Jabłońska A, Jabłonowska E, Studzińska M, Kamerys J, Paradowska E (2021) The TLR9 2848C/T Polymorphism Is Associated with the CMV DNAemia among HIV/CMV Coinfected Patients. Cells 10:2360. https://doi.org/10.3390/cells10092360
Ariyanto IA, Estiasari R, Waters S, Wulandari EAT, Fernandez S, Lee S, Price P (2018) Active and Persistent Cytomegalovirus Infections Affect T Cells in Young Adult HIV Patients Commencing Antiretroviral Therapy. Viral Immunol 31:472–479. https://doi.org/10.1089/vim.2018.0014
Duan T, Du Y, Xing C, Wang HY, Wang RF (2022) Toll-Like Receptor Signaling and Its Role in Cell-Mediated Immunity. Front Immunol 13:812774. https://doi.org/10.3389/fimmu.2022.812774
Brisse M, Ly H (2019) Comparative Structure and Function Analysis of the RIG-I-Like Receptors: RIG-I and MDA5. Front Immunol 10:1586. https://doi.org/10.3389/fimmu.2019.01586
Huik K, Avi R, Pauskar M, Kallas E, Jõgeda EL, Karki T, Marsh K, Des Jarlais D, Uusküla A, Lutsar I (2013) Association between TLR3 rs3775291 and resistance to HIV among highly exposed Caucasian intravenous drug users. Infect Genet Evol 20:78–82. https://doi.org/10.1016/j.meegid.2013.08.008
Sironi M, Biasin M, Cagliani R, Forni D, De Luca M, Saulle I, Lo Caputo S, Mazzotta F, Macías J, Pineda JA, Caruz A, Clerici M (2012) A common polymorphism in TLR3 confers natural resistance to HIV-1 infection. J Immunol 188:818–823. https://doi.org/10.4049/jimmunol.1102179
Hu J, Nistal-Villán E, Voho A, Ganee A, Kumar M, Ding Y, García-Sastre A, Wetmur JG (2010) A common polymorphism in the caspase recruitment domain of RIG-I modifies the innate immune response of human dendritic cells. J Immunol 185:424–432. https://doi.org/10.4049/jimmunol.0903291
Studzińska M, Jabłońska A, Wiśniewska-Ligier M, Nowakowska D, Gaj Z, Leśnikowski ZJ, Woźniakowska-Gęsicka T, Wilczyński J, Paradowska E (2017) Association of TLR3 L412F Polymorphism with Cytomegalovirus Infection in Children. PLoS ONE 12:e0169420. https://doi.org/10.1371/journal.pone.0169420
Paradowska E, Przepiórkiewicz M, Nowakowska D, Studzińska M, Wilczyński J, Emery VC, Leśnikowski ZJ (2006) Detection of cytomegalovirus in human placental cells by polymerase chain reaction. APMIS 114:764–771. https://doi.org/10.1111/j.1600-0463.2006.apm_31.x
Singh H, Samani D (2022) TLR3 polymorphisms in HIV infected individuals naïve to ART. Curr HIV Res 20:397–406. https://doi.org/10.2174/1570162X20666220908105434
Li P, Kaiser P, Lampiris HW, Kim P, Yukl SA, Havlir DV, Greene WC, Wong JK (2016) Stimulating the RIG-I pathway to kill cells in the latent HIV reservoir following viral reactivation. Nat Med 22:807–811. https://doi.org/10.1038/nm.4124
Kim Y, Anderson JL, Lewin SR (2018) Getting the Kill into Shock and Kill: Strategies to Eliminate Latent HIV. Cell Host Microbe 23:14–26. https://doi.org/10.1016/j.chom.2017.12.004
Garcia-Vidal E, Castellví M, Pujantell M, Badia R, Jou A, Gomez L, Puig T, Clotet B, Ballana E, Riveira-Muñoz E, Esté JA (2017) Evaluation of the Innate Immune Modulator Acitrecin as a Strategy To Clear the HIV Reservoir. Antimicrob Agents Chemother 61:e01368–e01317. https://doi.org/10.1128/AAC.01368-17
Chattopadhyay S, Sen GC (2014) dsRNA-activation of TLR3 and RLR signaling: gene induction-dependent and independent effects. J Interferon Cytokine Res 34:427–436. https://doi.org/10.1089/jir.2014.0034
Weck MM, Grünebach F, Werth D, Sinzger C, Bringmann A, Brossart P (2007) TLR ligands differentially affect uptake and presentation of cellular antigens. Blood 109:3890–3894. https://doi.org/10.1182/blood-2006-04-015719
Haralambieva IH, Ovsyannikova IG, Umlauf BJ, Vierkant RA, Pankratz VS, Jacobson RM, Poland GA (2011) Genetic polymorphisms in host antiviral genes: associations with humoral and cellular immunity to measles vaccine. Vaccine 29:8988–8997. https://doi.org/10.1016/j.vaccine.2011.09.043
Fry TJ, Mackall CL (2005) The many faces of IL-7: from lymphopoiesis to peripheral T cell maintenance. J Immunol 174:6571–6576. https://doi.org/10.4049/jimmunol.174.11.6571
Park JH, Yu Q, Erman B, Appelbaum JS, Montoya-Durango D, Grimes HL, Singer A (2004) Suppression of IL7Ralpha transcription by IL-7 and other prosurvival cytokines: a novel mechanism for maximizing IL-7-dependent T cell survival. Immunity 21:289–302. https://doi.org/10.1016/j.immuni.2004.07.016
Pasin C, Dufour F, Villain L, Zhang H, Thiébaut R (2018) Controlling IL-7 Injections in HIV-Infected Patients. Bull Math Biol 80:2349–2377. https://doi.org/10.1007/s11538-018-0465-8
Thiébaut R, Jarne A, Routy JP, Sereti I, Fischl M, Ive P, Speck RF, D’Offizi G, Casari S, Commenges D, Foulkes S, Natarajan V, Croughs T, Delfraissy JF, Tambussi G, Levy Y, Lederman MM (2016) Repeated Cycles of Recombinant Human Interleukin 7 in HIV-Infected Patients With Low CD4 T-Cell Reconstitution on Antiretroviral Therapy: Results of 2 Phase II Multicenter Studies. Clin Infect Dis 62:1178–1185. https://doi.org/10.1093/cid/ciw065
Acknowledgments
This work was supported by the Statutory Fund of the Institute of Medical Biology, Polish Academy of Sciences [Internal Grant of IMB of PAS for Young Researcher to A.J.]. The authors are grateful to all volunteers for their valuable contribution to the study.
Funding
This work was supported by the Statutory Fund of the Institute of Medical Biology, Polish Academy of Sciences [Internal Grant of IMB of PAS for Young Researcher to AJ].
Author information
Authors and Affiliations
Contributions
The study conception and design were done by Agnieszka Jabłońska and Edyta Paradowska. Material preparation and data collection were performed by Elżbieta Jabłonowska and Juliusz Kamerys, experiments were done by Agnieszka Jabłońska and Mirosława Studzińska, and all analyses were performed by Agnieszka Jabłońska. The first draft of the manuscript was written by Agnieszka Jabłońska, and all authors commented on previous versions of the manuscript. All authors read and approved the final manuscript.
Corresponding author
Ethics declarations
Ethical approval
This study was performed in accordance with the principles of the Declaration of Helsinki. Approval was granted by the ethics committee of the Medical University of Lodz (RNN/211/06/KE and RNN/33/17/KE).
Consent to participate
Informed consent was obtained from all individual participants included in the study.
Conflict of interest
The authors have no relevant financial or non-financial interests to disclose.
Additional information
Handling Editor Hugo Soudeyns
Publisher’s Note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Jabłońska, A., Jabłonowska, E., Studzińska, M. et al. Polymorphisms in the genes encoding RLR and TLR3 and CMV DNAemia in subjects coinfected with human immunodeficiency virus and cytomegalovirus. Arch Virol 169, 211 (2024). https://doi.org/10.1007/s00705-024-06114-3
Received:
Accepted:
Published:
DOI: https://doi.org/10.1007/s00705-024-06114-3