- Open Access
Cytosolic sulfotransferase 1A1 regulates HIV-1 minus-strand DNA elongation in primary human monocyte-derived macrophages
Virology Journalvolume 13, Article number: 30 (2016)
The cellular sulfonation pathway modulates key steps of virus replication. This pathway comprises two main families of sulfonate-conjugating enzymes: Golgi sulfotransferases, which sulfonate proteins, glycoproteins, glycolipids and proteoglycans; and cytosolic sulfotransferases (SULTs), which sulfonate various small molecules including hormones, neurotransmitters, and xenobiotics. Sulfonation controls the functions of numerous cellular factors such as those involved in cell-cell interactions, cell signaling, and small molecule detoxification. We previously showed that the cellular sulfonation pathway regulates HIV-1 gene expression and reactivation from latency. Here we show that a specific cellular sulfotransferase can regulate HIV-1 replication in primary human monocyte-derived macrophages (MDMs) by yet another mechanism, namely reverse transcription.
MDMs were derived from monocytes isolated from donor peripheral blood mononuclear cells (PBMCs) obtained from the San Diego Blood Bank. After one week in vitro cell culture under macrophage-polarizing conditions, MDMs were transfected with sulfotranserase-specific or control siRNAs and infected with HIV-1 or SIV constructs expressing a luciferase reporter. Infection levels were subsequently monitored by luminescence. Western blotting was used to assay siRNA knockdown and viral protein levels, and qPCR was used to measure viral RNA and DNA products.
We demonstrate that the cytosolic sulfotransferase SULT1A1 is highly expressed in primary human MDMs, and through siRNA knockdown experiments, we show that this enzyme promotes infection of MDMs by single cycle VSV-G pseudotyped human HIV-1 and simian immunodeficiency virus vectors and by replication-competent HIV-1. Quantitative PCR analysis revealed that SULT1A1 affects HIV-1 replication in MDMs by modulating the kinetics of minus-strand DNA elongation during reverse transcription.
These studies have identified SULT1A1 as a cellular regulator of HIV-1 reverse transcription in primary human MDMs. The normal substrates of this enzyme are small phenolic-like molecules, raising the possibility that one or more of these substrates may be involved. Targeting SULT1A1 and/or its substrate(s) may offer a novel host-directed strategy to improve HIV-1 therapeutics.
Host cellular machinery is exploited to facilitate all steps of HIV-1 replication. A new paradigm in the treatment of HIV-1 infection is to target these so-called host-derived dependency factors, as exemplified by CCR5 coreceptor antagonists . By contrast to the existing classes of direct-acting antivirals (DAAs) that target viral proteins, host-directed therapies may be less prone to the development of viral drug resistance and offer the potential for broader spectrum therapeutics [2, 3]. Therefore, there is currently a great deal of interest in better understanding the roles played by cellular factors and pathways during HIV-1 replication [4–8].
The cellular sulfonation pathway was first shown to play a key role in regulating HIV-1 infection at the level of cellular entry [9–13]. Previously, we uncovered another role for this pathway, demonstrating that it regulates retroviral transcription . In that study, a forward genetic screen implicated two specific bi-functional 3′-phosphoadenosine-5′phosphosulfate (PAPS) synthetase enzymes, PAPSS1 and PAPSS2, as being important for retroviral replication . These proteins catalyze two enzymatic steps to generate PAPS, the high-energy sulfonate-donor used in all cellular sulfonation reactions . This specific effect was demonstrated using two different inhibitors of the sulfonation pathway: chlorate, a substrate analog of sulfate that blocks PAPS formation; and guaiacol, a sulfotransferase substrate mimic [14, 16]. In addition, we have recently shown that treatment with these chemical inhibitors significantly blocks HIV-1 reactivation from latency in a primary human CD4+ T cell model and in established cell lines where latency is maintained by diverse regulatory mechanisms .
The cellular sulfonation system consists of a family of sulfotransferase enzymes that are responsible for sulfonate transfer within the cell . These proteins catalyze the transfer of a sulfuryl group (SO3 −) from PAPS to a hydroxyl or amino-group on an acceptor molecule. Sulfotransferases are organized into two main sub-families: the Golgi and cytosolic sulfotransferases. The Golgi sulfotransferases are membrane bound enzymes that sulfonate cell surface proteins, carbohydrates, proteoglycans, and glycoproteins, while the cytosolic sulfotransferases are cytoplasmic enzymes that sulfonate endogenous hormones, neurotransmitters, and small metabolites as well as exogenous xenobiotics (Fig. 1a). Cell surface sulfonation is necessary during normal homeostatic processes such as lymphocyte homing and cellular signaling [19–22]. Cytoplasmic sulfonation of metabolites by the cytosolic sulfotransferases (SULTs) generally leads to their inactivation, detoxification, and/or bioactivation [23–27]. Here we show that one of these cytosolic sulfotransferases, SULT1A1, regulates HIV-1 reverse transcription in MDMs, increasing our knowledge of the roles played by cellular factors in regulating HIV-1 reverse transcription.
Human cytosolic sulfotransferase 1A1 is highly expressed in primary human monocyte-derived macrophages
To determine if any of the 12 known cytosolic SULTs might play a role in regulating HIV-1 infection, we first compared their relative expression levels in the two physiologically relevant cell types, primary human CD4+ T cells and primary monocytic cells. We employed the publically available mRNA expression database Bio-GPS . This analysis revealed a strikingly high level of SULT1A1 mRNA in CD14+ monocytes as compared to other other cell types including CD4+ T cells (Additional file 1: Figure S1). Although SULT1A1 was previously found to be important in tissues such as the liver, brain, kidney, and gastrointestinal tract, little or nothing is known about its role in immune cells [29–31]. MDM-selective expression was confirmed by immunoblot analysis of protein lysates obtained from primary human CD4+ T cells and MDMs. In agreement with the mRNA expression data, SULT1A1 was highly expressed in MDMs. However, SULT1A1 protein expression was undetectable in resting or activated CD4+ T cells (Fig. 1b).
SULT1A1 knockdown decreases retroviral infection in MDMs
To test if SULT1A1 plays a role during retroviral infection in MDMs, siRNA knockdown was used to reduce the levels of this protein (Fig. 2a). Three distinct SULT1A1-targeting siRNAs (#1–3) each reduced SULT1A1 protein levels by 70–80 % at 96 h post-transfection as compared to a control (scrambled sequence) siRNA (Fig. 2b, c middle panel). Each of the 3 SULT1A1 siRNAs also reduced the levels of infection seen with a VSV-G-pseudotyped HIV-1 NL43 virus vector as judged by monitoring expression of the firefly luciferase reporter enzyme from the viral genome . Knockdown of SULT1A1 expression with SULT1A1 siRNAs 1, 2, or 3 resulted in a decrease in HIV-1 reporter gene expression by 50 % (p < 0.005), 76 % (p < 0.0005), and 57 % (p < 0.005), respectively (Fig. 2c, left panel). None of the siRNAs used significantly impacted cell viability (Fig. 2c, right panel). The fact that all three SULT1A1-directed siRNAs reduced viral gene expression following infection strongly argues against an indirect off-target effect being responsible for this effect.
To test if SULT1A1 could also influence infection by the related simian immunodeficiency virus, SULT1A1 siRNA-treated and control siRNA-treated MDMs were infected with a VSV-G-pseudotyped SIVagm virus vector encoding firefly luciferase (Fig. 2d) . As for HIV-1, RNAi-mediated knockdown of SULT1A1 directly correlated with a significant reduction in expression of the virus-encoded reporter enzyme, with an average of 85 % inhibition (p < 0.0005) (Fig. 2d, left panel).
To further validate the role of SULT1A1 during HIV-1 infection, we next investigated the impact of knocking down expression of this protein on infection of MDMs by replication-competent HIV-1. MDMs that were transfected with control siRNA or with SULT1A1-siRNA#2 were challenged with the replication-competent CCR5-tropic HIV-1 Env + JM1186 virus encoding Renilla luciferase [34, 35] and luciferase expression was assayed three days post infection (Fig. 3a). SULT1A1 knockdown was associated with a significant inhibition of virus-encoded luciferase expression in MDMs derived from multiple donors without affecting cell viability (Fig. 3). Transfection of these cells with SULT1A1 siRNA #2 resulted in an average 72 % decrease in HIV-1 reporter expression compared to control (p < 0.0005) (Fig. 3, left panel). Taken together, these results demonstrate that SULT1A1 is important for efficient virus gene expression following infection of MDMs with single cycle HIV-1 and SIV vectors and with replication-competent HIV-1.
SULT1A1 regulates HIV-1 reverse transcription
To determine the step in HIV-1 replication that is influenced by SULT1A1, we monitored the effect of SULT1A1 siRNA #2 on early steps of virus replication at 24 h post-infection. The VSV-G-pseudotyped HIV-1 vector was used for these studies to avoid multiple cycles of virus infection confounding the interpretation of the results. Quantitative PCR methods were used to monitor viral DNA and RNA products, focusing specifically upon spliced viral RNAs. These RNAs are produced de novo in infected cells and thus, are clearly distinguished from the large amounts of input unspliced viral genomic RNA that are present in these cells due to efficient virus uptake. Immunoblotting was used to monitor the expression levels of two independent viral proteins (Vpu and Vif), that are produced from spliced HIV-1 mRNA transcripts.
These studies revealed that SULT1A1 had no effect upon the levels of early reverse transcription products (defined as those generated prior to minus-strand DNA transfer) (Fig. 4a, left panel). By contrast, knockdown of SULT1A1 was associated with a reduction (58 %, p < 0.0005) in the levels of late reverse transcription products (defined here as those generated subsequent to minus-strand DNA transfer) (Fig. 4a, right panel). Consistently, SULT1A1 knockdown in MDMs was associated with a 72 % reduction in levels of HIV-1 multiply spliced RNA (forward and reverse primers span the first and second exons of Tat/Rev, respectively (p < 0.0005) (Fig. 4b). Furthermore, SULT1A1 knockdown was also correlated with a 70 % reduction in the levels of both the HIV-1 Vif and Vpu proteins (p < 0.0005) (Fig. 4c-d). Taken together, these results indicate that the predominant effect of SULT1A1 on HIV-1 replication is at the level of viral DNA synthesis.
SULT1A1 influences the kinetics of HIV-1 minus-strand DNA elongation
In order to determine the specific stage of HIV-1 reverse transcription that is influenced by SULT1A1, MDMs were transfected with SULT1A1-specific or control siRNA prior to infection with VSV-G pseudotyped NL43-Luc HIV-1 vector and DNA was isolated at different time points post-infection (ranging from 8–24 h). The relative abundance of different length reverse transcription products was then measured using a series of oligonucleotide primers that were used to amplify different regions of HIV-1 DNA (labeled in order of appearance as follows: ERT, U3-R, 2 KB, 4 KB, 8 KB, LRT (Fig. 5a).
Consistent with our previous result (Fig. 4), the abundance of early reverse transcription products (ERT and U3-R) was largely the same in both SULT1A1 siRNA transfected and control transfected cell populations (Fig. 5b all panels). By contrast, there was a marked reduction of DNA products longer than 2 kb in length at 8 h post-infection in cells deficient in SULT1A1 (Fig. 5b, left panel). The defect in 2 kb products was less pronounced at 16 h post-infection and was not evident at 24 h post-infection (Fig. 5b). Similarly the defect in the level of 4 kb products was less pronounced at 24 h as compared with 16 h post-infection. The defect seen in the levels of longer 8 kb and LRT products was not overcome in the 24-h time frame. Taken together, these results show that SULT1A1 knockdown is associated with a decreased progression of reverse transcription, a result that is consistent with this enzyme playing an important role during the kinetics of viral minus strand DNA elongation.
This study demonstrates that the cellular sulfotransferase SULT1A1 regulates HIV-1 reverse transcription in primary human monocyte-derived macrophages (MDMs). We showed that SULT1A1 is highly expressed in MDMs and that RNAi-mediated depletion of SULT1A1 in these cells results in a significant reduction in the kinetics of minus-strand DNA elongation during HIV-1 reverse transcription.
The synthesis of HIV-1 proviral DNA from the viral RNA genome is heavily regulated by cellular factors; however, only a small number of these factors have been well characterized to date [36–39]. These proteins include SAMHD1, which blocks reverse transcription in myeloid cells and resting CD4+ T cells by hydrolyzing dNTPs and/or degrading viral RNA [40–43], and APOBEC3G, which deaminates cytidine to uridine resulting in hypermutation during DNA synthesis [44, 45]. In addition, other factors have been shown to affect the kinetics of viral DNA synthesis . Thus, the studies described in this report extend our understanding of the roles of cellular factors in regulating this key step of retroviral replication. This novel role for SULT1A1 in the regulation of retroviral reverse transcription also adds to our growing knowledge about the diverse roles that the sulfonation pathway plays in the retroviral life cycle. For example, tyrosylprotein sulfotransferases 1 and 2 (TPST1 and TPST2) are Golgi sulfotransferases that sulfonate N-terminal tyrosine residues of CCR5 and enable efficient cellular entry of R5-tropic viruses [9, 10, 13]. It has also been demonstrated that HIV-1 binds to sulfonated proteoglycans on cell surfaces [11, 12]. In addition, we previously showed that PAPSS deficiency or treatment of cells with the sulfonation pathway inhibitors chlorate and guaiacol blocked HIV-1 de novo gene expression from the viral LTR promoter, and more recently we showed that these inhibitors also block HIV-1 reactivation from latency [14, 17]. Taken together, these observations demonstrate the importance of the sulfonation pathway at multiple steps of HIV-1 replication. It will be important for future studies to determine which sulfotranserase(s) regulate HIV-1 infection and reactivation from latency in CD4+ T cells, as SULT1A1 does not appear to be expressed at the protein level in these cells and control has been demonstrated at level of transcription, not reverse transcription, upon treatment with chlorate and guaiacol.
SULT1A1 is highly polymorphic within the human population, with both genetic polymorphisms and copy number variation conferring different levels of enzymatic activity [46–48]. Moreover, SULT1A1 variation has been linked to a number of diseases such as cancer [49–52], heart disease , and inflammatory bowel disease . Consequently, we are now seeking to determine if there is a correlation between SULT1A1 variability and HIV-1 susceptibility and/or AIDS disease progression.
Further investigation will be aimed at determining if SULT1A1 acts on HIV-1 through a substrate-dependent or -independent mechanism. It is possible that SULT1A1 may act independently of substrate by directly modifying viral proteins (such as reverse transcriptase). If the sulfonation of a specific SULT1A1 substrate is required, on the other hand, then identification of that substrate will be critical for understanding the underlying mechanism involved.
In summary, we demonstrated that a human cytosolic sulfotransferase, SULT1A1, regulates HIV-1 reverse transcription in human monocyte-derived macrophages (MDMs). We showed that SULT1A1 is highly expressed in primary human monocytes and MDMs. RNAi-knockdown of SULT1A1 in MDMs leads to a substantial decrease in infection by both pseudotyped and replication-competent HIV-1 vectors, as well as by a SIVagm vector. Quantitative PCR analysis revealed that this effect is associated with a defect in minus-strand DNA elongation during HIV-1 reverse transcription. These results support the idea that SULT1A1 is a novel HIV-1 host factor in MDMs, and suggest that targeting SULT1A1 or its substrate may lead to improved HIV-1 therapies.
AllStars Negative control and SULT1A1 Flexitube siRNAs (sequences provided in Additional file 2: Table S1) were obtained from Qiagen, reconstituted at 20 μM in water, and stored at −20 °C until use. Cell viability was assayed using Cell Titer-Glo reagent and luciferase activity was measured using Bright-Glo reagent according to the manufacturer’s instructions (Promega).
SULT mRNA expression analysis
The expression level for each cytosolic sulfotransferase in CD4+ T cells and CD14+ monocytes was derived from publically available expression data from BioGPS , and normalized to the median expression of that sulfotransferase in all tissues tested.
Peripheral blood mononuclear cells
Human donor buffy coats and LRS-WBC (white blood cells isolated in the Leuko-Reduction system via Terumo BCT Trima Automated Collection System) samples were collected from anonymous healthy donors and obtained from the San Diego Blood Bank. Written informed consent for the use of buffy coats and LRS samples for research purposes was obtained from the donors by the San Diego Blood Bank. Samples are routinely tested for the presence of HIV-1 antibodies and all samples used in the study are confirmed HIV-1 negative. Peripheral blood mononuclear cells (PBMCs) were isolated from these samples by Ficoll density gradient centrifugation. Briefly, buffy coats and LRS samples were diluted in RPMI, layered over Ficoll (Ficoll-Paque Plus, GE Healthcare), and centrifuged at 1850 rpm for 25 min without brakes. Cells at the interface were removed and washed twice in RPMI. Platelets were then removed by a final spin at 800 rpm without brakes. The cells were counted and resuspended at a density of 25x106 cells/ml in FBS supplemented with 10 % DMSO, transferred to −80 °C at least overnight, and then to liquid nitrogen for long-term storage.
CD4+ T cells
PBMCs were thawed in RPMI, washed, and CD4+ T cells were isolated using CD4+ negative selection magnetic bead isolation (EasySep Human CD4+ T cell enrichment kit, StemCell Technologies). Resting CD4+ T cells were lysed directly after separation, and the remaining CD4+ T cells were activated using CD3/CD28 beads for three days (Dynabeads Human T-Activator CD3/CD28, Life Technologies). CD4+ T cells were resuspended at 2x106 cells/100 μl 1× LDS lysis buffer (Invitrogen), diluted 1:3, and 10 μl lysate was loaded onto a gel 4–12 % Bis-Tris gel for immunoblot analysis.
PBMCs were thawed in RPMI, washed, and CD14+ monocytes were isolated using CD14 positive selection magnetic cell sorting according to the manufacturer’s instructions (Easy Sep Human CD14 Positive Selection kit, StemCell Technologies). CD14+ monocytes were plated at 5x106 cells per 10 cm polypropylene petri dish (Fisher) in RPMI 1640 medium (Gibco-BRL) supplemented with 10 % Human AB Serum (Sigma), 50 U/ml penicillin, 50 μg/ml streptomycin, 10 mM HEPES, sodium pyruvate, and 20 ng/ml recombinant human M-CSF (Peprotech). Fresh media without cytokine was added after 3–4 days, and by day 7 the MDMs were fully differentiated.
MDMs were washed with PBS, treated with Accutase (Stem Pro Accutase Cell Dissociation Reagent, Life Technologies) at 37 °C for 30 min, and dissociated by gentle pipetting. Cells were transfected with siRNA using the NEON electroporation system (Life Technologies) according to the manufacturer’s instructions. Briefly, 1.5×105 MDMs were mixed with 3 μl 20 μM siRNA in a 10 μl final reaction volume, electroporated with 2 pulses of 1500 V for 20 ms, and then transferred to 500 μl pre-warmed RPMI 10 % human serum without antibiotics in a 48 well plate and allowed to recover for 4 days. At 4 days post transfection, samples were assayed for protein knockdown by immunoblot. Samples with <60 % SULT1A1 knockdown and/or <65 % cell viability were not used in the analysis.
Viruses and infection
The HIV-1 NL43-Luc and SIVagm plasmids were obtained from Ned Landau [32, 33]. HIV-1 Env + JM1186-Rluc plasmid was made by Sumit Chanda’s lab by cloning the V3 loop of Gp120 from isolate 92TH014  and Renilla luciferase reporter into pBR-NL43-IRES-eGFP . VSV-G pseudotyped NL43-Luc HIV-1 and Env + JM1186-Rluc HIV-1 viruses were produced by transient transfection of 293 T cells by the Salk viral vector core, and VSV-G-pseudotyped SIVagm-Luc was produced in a similar method as previously described . HIV-1 and SIVagm viruses were assayed for p24 or p27 content, respectively, by p24 or p27 antigen capture ELISA according to the manufacturer’s instructions (Zeptometrix).
For MDM infection experiments, media was removed 96 h post transfection with siRNA, replaced with 100 μl virus (corresponding to 164 ng p24 VSV-G pseudotyped NL43-Luc HIV-1, 66.3 ng p24 Env + −JM1186-Rluc HIV-1, 234 ng p27 VSV-G pseudotyped SIVagm-Luc) diluted in 400 μl fresh RPMI 10 % human serum, and cells were spinoculated at 1200 × g for 60 min. Viral reporter expression and cell viability was assayed 24 h post infection for VSV-G-pseudotyped viruses, and 3 days post infection for replication competent HIV-1.
Immunoblot and protein quantitation
Cells were lysed in 1× LDS sample buffer (Invitrogen) and stored at −20 °C until use. Samples were thawed on ice, incubated at 95 °C for 5 min, and centrifuged for 3–5 min before loading. Precision Plus Protein Dual Color Standards (Bio-Rad) or Novex Sharp Pre-stained standards (Invitrogen) were used as protein standards, and 4–12 % Bis-Tris gels (Invitrogen) were used for gel electrophoresis. Protein was transferred onto PVDF membrane (Millipore Immobilon-FL) using BioRad wet transfer apparatus at 100 V for 1 h at 4 °C. Membranes were blocked with Casein blocking buffer (Bio-Rad) for at least 1 h at room temperature, then incubated with primary antibody diluted in 0.1 % Casein/0.2× PBS + 0.1 % Tween-20 overnight at 4 °C. Primary antibodies used in the study include mouse anti-human SULT1A1 mAb (clone 638708, R&D Systems) used at 1:2000 dilution, rabbit anti-HIV-1 Vif (clone A319, NIH AIDS Reagent program) used at 1:500, rabbit anti-HIV-1 Vpu (clone ab81532, Abcam) used at 1:1000 dilution, mouse anti-human Ku-86 mAb (clone B-1, Santa Cruz Biotechnology) used at 1:500 dilution, and anti-human mouse GAPDH (clone 6C5, Abcam) used at 1:5000. Membranes were washed three times with 1× PBS/ 0.1 % Tween-20, incubated with Alexa-Fluor 680-conjugated secondary antibody diluted in 0.1 % Casein 0.2× PBS 0.1 % Tween-20 and 0.01 % SDS at room temperature for at least 1 h. Secondary antibodies used in the study include goat anti-mouse Alexa-Fluor 680 IgG (H + L) (clone A21057, Invitrogen), and donkey anti-rabbit Alexa-Fluor 680 IgG (H + L) (clone A10043, Invitrogen). Membranes were washed three times with 1× PBS/ 0.1 % Tween 20, and imaged using the Licor Odyssey system. Protein expression was quantified using Image Studio software (Licor).
Detection of nucleic acids by real-time quantitative PCR
Total RNA was prepared using Qiazol lysis reagent (Qiagen) and miRNeasy RNA isolation kit (Qiagen) according to the manufacturer’s instructions. cDNA was synthesized using Quantitect Reverse Transcription kit (Qiagen) according to the manufacturer’s instructions. DNA was isolated from cells using a DNeasy Blood and Tissue Kit (Qiagen) according to the manufacturer’s instructions. Quantitation of ERT, LRT, and PBGD was performed using primers and probes diluted in TaqMan universal PCR master mix (Invitrogen). Amplification of other DNA products was monitored using SYBR green fluorescence (Invitrogen). Real-time PCR was performed using the ViiA 7 Real-time PCR system (Life Technologies). Standard curves were generated for all primers and efficiencies were found to be equivalent. Relative expression was calculated using the delta CT method as previously described . All primer and probe sequences used in the study are included in Additional file 2: Table S1.
peripheral blood mononuclear cell
Fatkenheuer G, Pozniak AL, Johnson MA, Plettenberg A, Staszewski S, Hoepelman AI, et al. Efficacy of short-term monotherapy with maraviroc, a new CCR5 antagonist, in patients infected with HIV-1. Nat Med. 2005;11:1170–2.
Schwegmann A, Brombacher F. Host-directed drug targeting of factors hijacked by pathogens. Sci Signal. 2008;1:re8.
Law GL, Korth MJ, Benecke AG, Katze MG. Systems virology: host-directed approaches to viral pathogenesis and drug targeting. Nat Rev Microbiol. 2013;11:455–66.
Bushman FD, Malani N, Fernandes J, D’Orso I, Cagney G, Diamond TL, et al. Host cell factors in HIV replication: meta-analysis of genome-wide studies. PLoS Pathog. 2009;5:e1000437.
Konig R, Zhou Y, Elleder D, Diamond TL, Bonamy GM, Irelan JT, et al. Global analysis of host-pathogen interactions that regulate early-stage HIV-1 replication. Cell. 2008;135:49–60.
Brass AL, Dykxhoorn DM, Benita Y, Yan N, Engelman A, Xavier RJ, et al. Identification of host proteins required for HIV infection through a functional genomic screen. Science. 2008;319:921–6.
Zhou H, Xu M, Huang Q, Gates AT, Zhang XD, Castle JC, et al. Genome-scale RNAi screen for host factors required for HIV replication. Cell Host Microbe. 2008;4:495–504.
Yeung ML, Houzet L, Yedavalli VS, Jeang KT. A genome-wide short hairpin RNA screening of jurkat T-cells for human proteins contributing to productive HIV-1 replication. J Biol Chem. 2009;284:19463–73.
Choe H, Li W, Wright PL, Vasilieva N, Venturi M, Huang CC, et al. Tyrosine sulfation of human antibodies contributes to recognition of the CCR5 binding region of HIV-1 gp120. Cell. 2003;114:161–70.
Farzan M, Mirzabekov T, Kolchinsky P, Wyatt R, Cayabyab M, Gerard NP, et al. Tyrosine sulfation of the amino terminus of CCR5 facilitates HIV-1 entry. Cell. 1999;96:667–76.
Mondor I, Ugolini S, Sattentau QJ. Human immunodeficiency virus type 1 attachment to HeLa CD4 cells is CD4 independent and gp120 dependent and requires cell surface heparans. J Virol. 1998;72:3623–34.
Roderiquez G, Oravecz T, Yanagishita M, Bou-Habib DC, Mostowski H, Norcross MA. Mediation of human immunodeficiency virus type 1 binding by interaction of cell surface heparan sulfate proteoglycans with the V3 region of envelope gp120-gp41. J Virol. 1995;69:2233–9.
Seibert C, Cadene M, Sanfiz A, Chait BT, Sakmar TP. Tyrosine sulfation of CCR5 N-terminal peptide by tyrosylprotein sulfotransferases 1 and 2 follows a discrete pattern and temporal sequence. Proc Natl Acad Sci U S A. 2002;99:11031–6.
Bruce JW, Ahlquist P, Young JA. The host cell sulfonation pathway contributes to retroviral infection at a step coincident with provirus establishment. PLoS Pathog. 2008;4:e1000207.
Klaassen CD, Boles JW. Sulfation and sulfotransferases 5: the importance of 3′-phosphoadenosine 5′-phosphosulfate (PAPS) in the regulation of sulfation. FASEB J. 1997;11:404–18.
Hortin GL, Schilling M, Graham JP. Inhibitors of the sulfation of proteins, glycoproteins, and proteoglycans. Biochem Biophys Res Commun. 1988;150:342–8.
Murry JP, Godoy J, Mukim A, Swann J, Bruce JW, Ahlquist P, et al. Sulfonation pathway inhibitors block reactivation of latent HIV-1. Virology. 2014;471-473C:1–12.
Chapman E, Best MD, Hanson SR, Wong CH. Sulfotransferases: structure, mechanism, biological activity, inhibition, and synthetic utility. Angew Chem Int Ed Engl. 2004;43:3526–48.
Hemmerich S, Rosen SD. Carbohydrate sulfotransferases in lymphocyte homing. Glycobiology. 2000;10:849–56.
Nadanaka S, Ishida M, Ikegami M, Kitagawa H. Chondroitin 4-O-sulfotransferase-1 modulates Wnt-3a signaling through control of E disaccharide expression of chondroitin sulfate. J Biol Chem. 2008;283:27333–43.
Kramer KL, Yost HJ. Heparan sulfate core proteins in cell-cell signaling. Annu Rev Genet. 2003;37:461–84.
Kawashima H, Petryniak B, Hiraoka N, Mitoma J, Huckaby V, Nakayama J, et al. N-acetylglucosamine-6-O-sulfotransferases 1 and 2 cooperatively control lymphocyte homing through L-selectin ligand biosynthesis in high endothelial venules. Nat Immunol. 2005;6:1096–104.
Allali-Hassani A, Pan PW, Dombrovski L, Najmanovich R, Tempel W, Dong A, et al. Structural and chemical profiling of the human cytosolic sulfotransferases. PLoS Biol. 2007;5:e97.
Hildebrandt MA, Carrington DP, Thomae BA, Eckloff BW, Schaid DJ, Yee VC, et al. Genetic diversity and function in the human cytosolic sulfotransferases. Pharmacogenomics J. 2007;7:133–43.
Falany CN. Enzymology of human cytosolic sulfotransferases. FASEB J. 1997;11:206–16.
Glatt H. Sulfotransferases in the bioactivation of xenobiotics. Chem Biol Interact. 2000;129:141–70.
Gamage N, Barnett A, Hempel N, Duggleby RG, Windmill KF, Martin JL, et al. Human sulfotransferases and their role in chemical metabolism. Toxicol Sci. 2006;90:5–22.
Wu C, Orozco C, Boyer J, Leglise M, Goodale J, Batalov S, et al. BioGPS: an extensible and customizable portal for querying and organizing gene annotation resources. Genome Biol. 2009;10:R130.
Riches Z, Stanley EL, Bloomer JC, Coughtrie MW. Quantitative evaluation of the expression and activity of five major sulfotransferases (SULTs) in human tissues: the SULT “pie”. Drug Metab Dispos. 2009;37:2255–61.
Salman ED, Kadlubar SA, Falany CN. Expression and localization of cytosolic sulfotransferase (SULT) 1A1 and SULT1A3 in normal human brain. Drug Metab Dispos. 2009;37:706–9.
Teubner W, Meinl W, Florian S, Kretzschmar M, Glatt H. Identification and localization of soluble sulfotransferases in the human gastrointestinal tract. Biochem J. 2007;404:207–15.
Connor RI, Chen BK, Choe S, Landau NR. Vpr is required for efficient replication of human immunodeficiency virus type-1 in mononuclear phagocytes. Virology. 1995;206:935–44.
Mariani R, Chen D, Schrofelbauer B, Navarro F, Konig R, Bollman B, et al. Species-specific exclusion of APOBEC3G from HIV-1 virions by Vif. Cell. 2003;114:21–31.
Munch J, Rajan D, Schindler M, Specht A, Rucker E, Novembre FJ, et al. Nef-mediated enhancement of virion infectivity and stimulation of viral replication are fundamental properties of primate lentiviruses. J Virol. 2007;81:13852–64.
Bjorndal A, Deng H, Jansson M, Fiore JR, Colognesi C, Karlsson A, et al. Coreceptor usage of primary human immunodeficiency virus type 1 isolates varies according to biological phenotype. J Virol. 1997;71:7478–87.
Warren K, Warrilow D, Meredith L, Harrich D. Reverse Transcriptase and Cellular Factors: Regulators of HIV-1 Reverse Transcription. Viruses. 2009;1:873–94.
Friedrich BM, Dziuba N, Li G, Endsley MA, Murray JL, Ferguson MR. Host factors mediating HIV-1 replication. Virus Res. 2011;161:101–14.
Arhel N, Kirchhoff F. Host proteins involved in HIV infection: new therapeutic targets. Biochim Biophys Acta. 1802;2010:313–21.
Goff SP. Host factors exploited by retroviruses. Nat Rev Microbiol. 2007;5:253–63.
Laguette N, Sobhian B, Casartelli N, Ringeard M, Chable-Bessia C, Segeral E, et al. SAMHD1 is the dendritic- and myeloid-cell-specific HIV-1 restriction factor counteracted by Vpx. Nature. 2011;474:654–7.
Hrecka K, Hao C, Gierszewska M, Swanson SK, Kesik-Brodacka M, Srivastava S, et al. Vpx relieves inhibition of HIV-1 infection of macrophages mediated by the SAMHD1 protein. Nature. 2011;474:658–61.
Baldauf HM, Pan X, Erikson E, Schmidt S, Daddacha W, Burggraf M, et al. SAMHD1 restricts HIV-1 infection in resting CD4(+) T cells. Nat Med. 2012;18:1682–7.
Ryoo J, Choi J, Oh C, Kim S, Seo M, Kim SY, et al. The ribonuclease activity of SAMHD1 is required for HIV-1 restriction. Nat Med. 2014;20:936–41.
Yu X, Yu Y, Liu B, Luo K, Kong W, Mao P, et al. Induction of APOBEC3G ubiquitination and degradation by an HIV-1 Vif-Cul5-SCF complex. Science. 2003;302:1056–60.
Sheehy AM, Gaddis NC, Malim MH. The antiretroviral enzyme APOBEC3G is degraded by the proteasome in response to HIV-1 Vif. Nat Med. 2003;9:1404–7.
Yu X, Dhakal IB, Beggs M, Edavana VK, Williams S, Zhang X, et al. Functional genetic variants in the 3′-untranslated region of sulfotransferase isoform 1A1 (SULT1A1) and their effect on enzymatic activity. Toxicol Sci. 2010;118:391–403.
Hebbring SJ, Adjei AA, Baer JL, Jenkins GD, Zhang J, Cunningham JM, et al. Human SULT1A1 gene: copy number differences and functional implications. Hum Mol Genet. 2007;16:463–70.
Ning B, Nowell S, Sweeney C, Ambrosone CB, Williams S, Miao X, et al. Common genetic polymorphisms in the 5′-flanking region of the SULT1A1 gene: haplotypes and their association with platelet enzymatic activity. Pharmacogenet Genomics. 2005;15:465–73.
Wang Y, Spitz MR, Tsou AM, Zhang K, Makan N, Wu X. Sulfotransferase (SULT) 1A1 polymorphism as a predisposition factor for lung cancer: a case-control analysis. Lung Cancer. 2002;35:137–42.
Nowell S, Ratnasinghe DL, Ambrosone CB, Williams S, Teague-Ross T, Trimble L, et al. Association of SULT1A1 phenotype and genotype with prostate cancer risk in African-Americans and Caucasians. Cancer Epidemiol Biomarkers Prev. 2004;13:270–6.
Zheng L, Wang Y, Schabath MB, Grossman HB, Wu X. Sulfotransferase 1A1 (SULT1A1) polymorphism and bladder cancer risk: a case-control study. Cancer Lett. 2003;202:61–9.
Tang D, Rundle A, Mooney L, Cho S, Schnabel F, Estabrook A, et al. Sulfotransferase 1A1 (SULT1A1) polymorphism, PAH-DNA adduct levels in breast tissue and breast cancer risk in a case-control study. Breast Cancer Res Treat. 2003;78:217–22.
O’Halloran AM, Patterson CC, Horan P, Maree A, Curtin R, Stanton A, et al. Genetic polymorphisms in platelet-related proteins and coronary artery disease: investigation of candidate genes, including N-acetylgalactosaminyltransferase 4 (GALNT4) and sulphotransferase 1A1/2 (SULT1A1/2). J Thromb Thrombolysis. 2009;27:175–84.
Imielinski M, Baldassano RN, Griffiths A, Russell RK, Annese V, Dubinsky M, et al. Common variants at five new loci associated with early-onset inflammatory bowel disease. Nat Genet. 2009;41:1335–40.
Konig R, Chiang CY, Tu BP, Yan SF, DeJesus PD, Romero A, et al. A probability-based approach for the analysis of large-scale RNAi screens. Nat Methods. 2007;4:847–9.
Schmittgen TD, Livak KJ. Analyzing real-time PCR data by the comparative C(T) method. Nat Protoc. 2008;3:1101–8.
We thank members of the Young lab for helpful discussion, especially John Naughton. This project was supported by a Salk-Sanofi innovation grant, the NIH Cellular and Molecular Training Grant, the Bruce J. Heim Foundation, the Jesse and Caryl Philips Foundation, the James B. Pendleton Charitable Trust, the NCI Cancer Center Support Grant Award, and for funding and support. We would also like to thank Kevin Olivieri and Manqing Li for helpful discusion and reagents, and the Salk Gene Transfer, Targeting, and Therapeutics Core (GT3) for lentivirus production.
The authors declare that they have no competing interests.
JS designed and conducted the experiments, analyzed the data, and wrote the manuscript. JM initiated the study, assisted in experimental design, discussed results, and wrote the manuscript. JY designed the experiments, analyzed data, and wrote the manuscript. All authors’s read and approved the final manuscript.
SULT1A1 is highly expressed in monocytes. The expression level for each cytosolic sulfotransferase in CD4+ T cells and CD14+ monocytes was derived from publically available expression data from BioGPS and normalized to the median expression of that sulfotransferase in all tissues tested. (PDF 26 kb)
Primer and siRNA sequences. DNA and RNA primer sequences used in the study are listed from 5′ to 3′. siRNAs are listed with the siRNA name, Qiagen ID, and sequences from 5′ to 3′. (XLSX 43 kb)