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G-quadruplexes are four-stranded conformations of nucleic acids that act as cellular epigenetic regulators. A dynamic G-quadruplex forming region in the HIV-1 LTR promoter represses HIV-1 transcription when in the folded conformation. This activity is enhanced by nucleolin, which induces and stabilizes the HIV-1 LTR G-quadruplexes. In this work by a combined pull-down/mass spectrometry approach, we consistently found hnRNP A2/B1 as an additional LTR-G-quadruplex interacting protein. Surface plasmon resonance confirmed G-quadruplex specificity over linear sequences and fluorescence resonance energy transfer analysis indicated that hnRNP A2/B1 is able to efficiently unfold the LTR G-quadruplexes. Evaluation of the thermal stability of the LTR G-quadruplexes in different-length oligonucleotides showed that the protein is fit to be most active in the LTR full-length environment. When hnRNP A2/B1 was silenced in cells, LTR activity decreased, indicating that the protein acts as a HIV-1 transcription activator. Our data highlight a tightly regulated control of transcription based on G-quadruplex folding/unfolding, which depends on interacting cellular proteins. These findings provide a deeper understanding of the viral transcription mechanism and may pave the way to the development of drugs effective against the integrated HIV-1, present both in actively and latently infected cells.
G-quadruplexes (G4s) are unique four-stranded nucleic acid structures that may form in guanine-rich sequences. Based on the strand orientation, they can adopt three main topologies: parallel, antiparallel, and hybrid-type structures. G4s have been shown to be involved in key regulatory and pathological roles in eukaryotes, including transcriptional regulation of gene promoters and enhancers, translation, chromatin epigenetic regulation, DNA recombination1,2,3. Formation of G4 in vivo has been consolidated by the development of G4 specific antibodies4,5.
Recently, the presence of G4s in viruses and their involvement in key steps of viral infection has been provided6. G4s have been reported in the SARS coronavirus7, the human papilloma, hepatitis C, Zika and Ebola virus genomes8,9,10,11. Among herpesviruses, RNA G4s have been implicated in the regulation of DNA replication and translation of the Epstein–Barr virus12,13. We have shown that the herpes simplex virus 1 possesses several repeats of sequences forming stable G4s, which were visualized in infected cells by a G4-specific antibody14; stabilization of these tetraplex structures by a G4 ligand inhibited viral DNA replication15.
The largest body of evidence of G4-mediated regulation of viruses has been provided for the human immunodeficiency virus-1 (HIV-1), the etiologic agent of the acquired immune deficiency syndrome (AIDS). We and other groups have identified functionally significant G4s in the Nef coding region16 and in the unique long terminal repeat (LTR) promoter17,18,19 of HIV-1. When the HIV-1 G4s were stabilized by G4 ligands, antiviral effects, mainly dependent on inhibition of LTR-mediated transcription, were observed18,20,21. Furthermore, the cellular protein nucleolin has been shown to stabilize the HIV-1 LTR G4s and induce potent inhibition of viral transcription22.
In general, several proteins that modulate G4s and/or serve as a bridge to recruit additional protein regulators have been reported23. Besides the shelterin complex proteins that are involved in telomere homeostasis24, G4 interacting proteins either stabilize (e.g. nucleolin, MAZ and nucleophosmin) or unfold (the helicase and heterogeneous nuclear ribonucleoprotein (hnRNP) families)25,26 the G4 conformation to allow for a tightly controlled modulation of the epigenetic G4 switch.
By means of mass spectrometry, surface plasmon resonance (SPR), fluorescence energy transfer (FRET), Taq polymerase stop and reporter assays, we here identified and characterized G4-selectivity and function of the hnRNP A2/B1, the first protein shown to unfold G4s in the HIV-1 LTR promoter.
We have shown that the HIV-1 LTR promoter can fold into three mutually exclusive G4s and that nucleolin, the most abundant nucleolar protein, can bind, induce and stabilize the LTR G4s22. We reasoned that other proteins may exist that regulate the G4/ds equilibrium at the LTR: we thus looked for additional proteins by pull-down assay of 293T nuclear cell extracts against the whole region in the HIV-1 LTR that can fold into G4, i.e. LTR-II+III+IV. This region can alternatively fold into three G4s, i.e. LTR-II, LTR-III and LTR-IV. As control, a two-point mutation LTR-II+III+IV oligonucleotide, which has been previously shown to be unable to fold into G4, i.e. LTR-II+III+IV M4+5, was used (Fig. 1a and Supplementary Table S1)18. After washing at increasing ionic strength to destabilize weak protein-G4 interactions, the final eluted sample was run on SDS-PAGE and subjected to MS analysis. A series of heterogeneous nuclear ribonucleoproteins (hnRNPs) were found to be present only in the G4-folded oligonucleotide (Table 1); among them, only hnRNP A2/B1 was obtained in all three independent tests, even if it did not obtain the highest score within each experiments (Fig. 1b). The identity and selectivity of hnRNP A2/B1 was confirmed by pull-down assay followed by western blot analysis with an anti-hnRNP A2/B1 antibody. The G4-folded LTR-II+III+IV was used along with the G-rich non-G4 forming LTR-II+III+IV M4+5 and a random oligonucleotide of the same length (Supplementary Table S1). The hnRNP A2/B1 protein was confirmed to bind mainly to the G4-folded sequence, even if in these settings it displayed mild recognition also of the G-rich non-G4-folding oligonucleotide (Fig. 1c). To confirm selectivity toward the G4 LTR oligonucleotide, surface plasmon resonance (SPR) analysis was performed. The recombinant purified hnRNP A2, which lacks 12 amino acids in the amino-terminal region and is the main isoform, accounting for ~90% of the protein in most tissues27, was immobilized on a SPR chip and binding affinity of the unlabelled oligonucleotides was measured. LTR-II+III+IV displayed the highest KD (19.5±1.5nM), while the mutant LTR-II+III+IV M4+5 was bound with a lower affinity (KD 35.5±3.0nM). Chi2 and U-values were <10 and <15, respectively, indicating optimal data fitting28,29. In contrast, binding to a random oligonucleotide of the same length as LTR-II+III+IV was so low that in these conditions it was not possible to obtain a meaningful KD value (Fig. 2).
We next set out to investigate the effect of hnRNP A2 binding to the LTR G4s. A Taq polymerase stop assay was performed on the LTR-II+III+IV template. In the presence of 100mMK+, stop sites corresponding to formation of LTR-III and LTR-II were visible (compare lanes 1 and 2, Fig. 3a). No stop corresponding to LTR-IV was detected, as expected, since LTR-IV has been previously reported to form upon induction by G4 ligands18. Upon addition of hnRNP A2, both LTR-III and LTR-II stop sites showed an insignificant decrease (compare lanes 3 and 2, Fig. 3a and b). Similarly, no effect was induced by addition of K+ and hnRNP A2 in the control LTR-II+III+IV M4+5 template lacking the possibility to form G4 (lanes 5–7, Fig. 3a).
As suggested by Xodo30, the apparent lack of effect in the presence of an unfolding protein could be due to the protein binding to the template sequence which would stimulate polymerase stop and mask G4 release at the same binding site. We thus switched to a dual-labelled system where oligonucleotide folding could be monitored by changes in fluorescence. Fluorescence resonance energy transfer (FRET) is a spectroscopic technique that provides information about structure and dynamics of nucleic acids folding. It involves a donor fluorophore in an excited state, the excitation energy of which can be transferred to a proximal acceptor chromophore. Given that the major determinant of FRET efficiency is the distance between the acceptor and the donor, fluorescence intensities depict nucleic acids folding states. Consequently, when annealed to its complementary sequence to form a double-stranded structure, the tested oligonucleotide would yield the maximum fluorescence intensity, while the G4 folded conformation would be the least fluorescent. In these conditions the measured fluorescence intensity allows to calculate the energy transfer (E) and the end-to-end distance (R) between the two fluorophores, and therefore the unfolding degree. The G4 folded LTR-II+III+IV sequence was characterized by R of ~38, with E ~0.84. When the G4 structure was converted into the duplex conformation by addition of the complementary C-rich strand, the fluorophores were separated by ~150, and FRET was approximately 0. Treatment of LTR-II+III+IV G4 with hnRNP A2 increased fluorescence by 3-folds with respect to the free G4, and E decreased to 0.51 (Fig. 4a and b, Supplementary Table S2). Considering that the complete unfolding of the G4 structure required ΔE=0.72, the ΔE=0.30 induced by hnRNP A2 reflected a 42% unfolding (Fig. 4c). The negative control protein BSA showed negligible unfolding activity in these conditions (Fig. 4c and Supplementary Table S2). To test the statistical significance of the effect observed in the presence of the protein, we applied a model comparison approach, which allows to test the statistical role of an independent variable (in our case the hnRNP A2 protein) through the comparison of two models differing only in that variable. The test yielded F (2, 189)=36.27 and P<0.0531, indicating that the difference observed in the presence and absence of the protein was statistically significant. Analysis of the activity of hnRNP A2 was extended to shorter LTR sequences, i.e. LTR-III+IV, LTR-III and LTR-IV G4s, folded in 100mMK+. The unfolding of LTR-III+IV and LTR-IV was similar but lower than that on the full-length sequence (31%); unfolding of LTR-III was very low (8.5%) (Fig. 4c, Supplementary Table S1 and Supplementary Fig. S2–S4) When the G4-forming sequences were folded in lower K+ concentrations, i.e. 50 and 25mM, a distinct enhancement of unfolding was observed: unfolding up to 83% was obtained in the LTR-II+III+IV oligonucleotide (Fig. 4c, Supplementary Table S1 and Supplementary Fig. S1).
Because G4s are less stable at lower K+ concentrations, we proposed that the diverse unfolding efficiency towards the different-length LTR G4s depended on the stability of the LTR G4s. To test this hypothesis, melting temperatures (Tm) of the dual-labelled oligonucleotides were thus measured by FRET-monitored thermal unfolding (Table 2). The most stable sequence was LTR-III (Tm 62.1±0.1°C), followed by LTR-IV and LTR-III+IV (Tm 59.1±0.1°C and 55.2±0.1°C, respectively); LTR-II+III+IV was the least stable sequence (Tm 49.1±0.1), confirming that the observed unfolding scale depended on the oligonucleotide stability in the FRET system. To note that in the unlabelled oligonucleotides measured by circular dichroism (CD), LTR-IV was the least stable sequence (Table 2), bias which likely derives by the absence of fluorophores at the oligonucleotides’ 5′- and 3′-end, which affect Tm values, as previously noted32.
In addition, the longest sequences, i.e. LTR-II+III+IV and LTR-III+IV, where multiple G4s may form, display Tm values that represent the average stability, which depends on the effective formation of the possible G4s. We thus performed a Taq polymerase stop assay to assess the G4 mutual formation and stability at increasing K+ concentration in the full-length LTR. LTR-III was used as a control sequence where only one G4 could form. We observed that in the full-length LTR-II+III+IV sequence, both LTR-II and LTR-III G4s formed upon addition of K+ (lanes 2–3, Fig. 5a); of these, LTR-III G4 induced a slightly more intense stop than LTR-II, suggesting a preferred formation of LTR-III in the full-length sequence (Fig. 5b). LTR-III was also the only G4 forming in the LTR-III+IV template (lanes 5–7, Fig. 5a). Interestingly, the LTR-III that formed in the full-length sequence was less intense than LTR-III forming in the shortest oligonucleotides (compare lanes 2–3, with 6–7 and 9–10, Fig. 5a and b). These data indicate that i) LTR-III is the most prominent G4 among the mutually exclusive LTR G4s and ii) when LTR-III forms in the full-length LTR promoter, its stability maintains a level that is fully susceptible to hnRNP A2 processing.
We have shown that LTR G4 folding inhibits viral transcription, whereas when point mutations that disrupt G4s are introduced in the LTR promoter, an increase in promoter activity is evidenced18. Silencing of the LTR G4 folding/stabilizing protein nucleolin significantly increased promoter activity, indicating the inhibitory effect of nucleolin on LTR-driven transcription22. To assess the effect of hnRNP A2/B1 binding/unfolding of the full-length LTR G4s, a set of anti-hnRNP A2/B1 siRNAs was used, which effectively silenced hnRNP A2/B1 expression in 293T cells (Fig. 6a). In these conditions, LTR-driven transcription decreased by 45% at the highest siRNA concentration in the wt LTR sequence (Fig. 6b). In contrast, the LTR sequence with two point mutations that disrupt G4 folding was only marginally affected by hnRNP A2/B1 depletion (Fig. 6b), indicating that the effect was G4-specific. In these conditions, hnRNP A2/B1-silenced 293T cells showed no reduction in cell viability at 48h with respect to the controls, thus confirming the consistency of the inhibitory effects on LTR promoter activity. Silencing of hnRNP A2/B1 was also performed in the TZM-bl reporter cell line, which contains stably integrated copies of the luciferase gene under control of the LTR wt promoter and thus closely resembles the integrated provirus. The LTR-driven reporter transcription decreased up to 33% in hnRNP A2/B1-silenced cells (Supplementary Fig. S5). These data further confirm the unfolding activity of hnRNP A2/B1 on the LTR G4s.
We have shown that hnRNP A2/B1 selectively binds the HIV-1 LTR G4s and unfolds them. While hnRNPs are RNA/protein complexes that bind newly synthesized RNA (pre-mRNA) in the cell nucleus during gene transcription and post-transcriptional modifications33, two of the most abundant of them, hnRNP A1 and hnRNP A2/B1, have been reported to bind also DNA in the quadruplex conformation. Initially hnRNP A1 was found to unfold the telomeric G4s and promote telomerase activity34,35,36, to unfold the G4 in the promoter of the KRAS oncogene and regulate transcription30 and to destabilize the tetraplex forms of the fragile X expanded sequence d(CGG)n37. HnRNP A2 has been shown to unfold the fragile X repeats38 and the shorter hnRNP A2 splice variant to promote telomere extension in mammalian cells39.
Our finding that hnRNP A2 binds and unfolds the G4s in the promoter of HIV-1 not only confirms the DNA G4 unfolding activity of this protein, but also indicates for the first time that this type of activity is exploited by a virus.
In HIV-1, hnRNP A2/B1 has been reported to play with Rev an important accessory role in promoting nuclear viral RNA retention and nucleocytoplasmic viral RNA transport40. In this context, the lower virus production observed upon siRNA-mediated depletion of hnRNP A2/B1 in infected cells was ascribed to accumulation of viral genomic RNA in cytoplasmic compartments or in the nucleus41. Our results showing decreased transcriptional activity upon depletion of hnRNP A2/B1 indicate a possible additional mechanism of inhibition of virus production mediated by increased G4 folding in the HIV-1 LTR promoter in the absence of hnRNP A2/B1. Surprisingly, overexpression of this protein and other hnRNP members induced similar effects, i.e. inhibition of transcription and reduction of virus production42. We suggest that upon stimuli that boost viral transcription (i.e. integral release of LTR G4s upon hnRNP A2/B1 massive overexpression) the virus (or the cell) activates counteracting mechanisms to avoid excessive exploitation of the cell by the virus that would lead to fast cell death, in the end impairing virus production. Therefore, the reported transcription inhibition might be mediated by other factors triggered by hnRNP A2/B1 overexpression.
The activity of hnRNP A2/B1 is fit to unfold the G4s that actually form in the HIV-1 LTR region. In fact, G4s folded in short oligonucleotides, such as LTR-III and LTR-IV, which displayed higher thermal stability, were only partially unfolded by the protein. In contrast, the same G4 structures folding in a longer context (LTR-II+III+IV) were less stable and were effectively processed by hnRNP A2/B1. Obviously, the longer oligonucleotide better mimes the actual G4 condition in the full-length LTR, as also proved by transcription inhibition obtained by hnRNP A2/B1 depletion in cells that contained the entire HIV-1 LTR.
The LTR G4 system displays regulating features similar to those described for the c-myc43,44, HRAS26 and KRAS oncogene-promoters30,45,46,47. As in these eukaryotic G4-modulated promoters, the HIV-1 LTR promoter is processed by G4 stabilizing (nucleolin)22 and destabilizing proteins (hnRNP A2/B1). Because the LTR promoter has been suggested to be the region where viral latency is regulated48,49, the G4 switch may play a role not only in activation of effective viral transcription, but also in its shift to latency. Currently, only the actively transcribed virus is targeted by antiviral drugs, while eradication of the HIV-1 infection has been made impossible by the existence of reservoirs of the latent virus50. Therefore, our findings not only advance our understanding on the mechanism of viral transcription but may also constitute a progress from a therapeutic point of view.
All desalted oligonucleotides were purchased from Sigma-Aldrich, Milan, Italy (Supplementary Table S1). TZM-bl (obtained through the NIH AIDS Reagent Program, Division of AIDS, NIAID, NIH, from Dr. J.C. Kappes, Dr. X. Wu, and Tranzyme Inc.) is a HeLa cell line stably expressing large amounts of CD4 and CCR5 and containing integrated copies of the luciferase and β-galactosidase genes under control of the HIV-1 promoter. Human embryonic kidney (HEK) 293T (ATCC # CRL-3216) and TZM-bl cells were grown in DMEM (Gibco, Thermo Fisher Scientific, Waltham, MA, USA) supplemented with 10% heat-inactivated fetal bovine serum (FBS, Gibco, Thermo Fisher Scientific, Waltham, MA, USA). Cells were grown in a humidified incubator maintained at 37°C with 5% CO2.
Protein nuclear extracts of HEK 293T cells were obtained by using NXTRACT kit (Sigma-Aldrich, Milan, Italy). HEK 293T protein nuclear extracts (150μg) were incubated with biotinylated LTR-II+III+IV G4, mutated M4+5 and random R oligonucleotides folded (600nM) in 250μl of reaction containing Tris-HCl 20mM, pH 8, KCl 30mM, MgCl2 1.5mM, protease inhibitor cocktail (Sigma-Aldrich, Milan, Italy) 1%, NaF 5mM, Na3VO4 (Sigma-Aldrich, Milan, Italy) 1mM, poly [dI-dC] (Sigma-Aldrich, Milan, Italy) 1.25ng/μl for 2h at 37°C. The binding reaction was followed by incubation (2h at 37°C) with 30μl of streptavidin-agarose beads (Sigma-Aldrich, Milan, Italy). After PBS and NaCl washes (0.2 and 1M), beads were collected by brief centrifugation, resuspended in 50μl of Laemmli buffer, and finally incubated at 95°C for 5min. Supernatants were separated in 12% SDS-PAGE and, after coomassie staining, the gel lanes of LTR G4 and LTR M4+5 were directly in-gel digested and analysed for protein identification by mass spectrometry (MS) (see MS protein identification in ref. 22). Briefly, gel lanes cut in ~0.5cm pieces were first washed with 50% CH3OH and 2.5% acetic acid, dehydrated with CH3CN, then reduced with 30μl of DTT (10mM in 100mM NH4HCO3) for 30min at room temperature; the excess of DTT was next neutralized by alkylation with 30μl of iodoacetamide (50mM in 100mM NH4HCO3) for 30min at room temperature. Bands were washed with 100mM NH4HCO3, dehydrated with CH3CN twice, and then digested overnight with 1μg of MS-grade trypsin (ThermoFisher Scientific, Waltham, MA, USA) in 50μl of 50mM NH4HCO3. Peptides were extracted twice with 5% formic acid and twice with 50% CH3CN/5% formic acid. The peptide mixture was further desalted in a silica nanocolumn (Polymicro Technologies, Phoenix, AZ, USA) packed in house with pinnacle C18 pack material (Thermo Fisher Scientific, Waltham, MA, USA). The desalted mixture was finally analyzed by direct infusion electrospray ionization (ESI) on a Thermo Fisher Scientific (Waltham, MA, USA) LTQ-Orbitrap Velos mass spectrometer utilizing quartz emitters produced in house. A stainless steel wire was inserted through the back-end of the emitter to supply an ionizing voltage that ranged between 0.8 and 1.2kV. Putative peptides present in wt LTR-II+III+IV (but not in M4+5) samples were submitted to tandem mass spectrometric (MS/MS) analysis. The masses of the 50 most intense fragment ions were employed to perform a Mascot Database Search51 to identify their parent protein. Significant Mascot hits were accepted as positive matches and their ion score reported (see MS protein identification in ref. 22 for more details). Supernatants were further analysed by Western blot with an anti-hnRNP A2/B1 antibody (mouse monoclonal DP3B3; Santa Cruz Biotechnology, Dallas, TX, USA).
SPR was performed on the Biacore T100 platform (GE Healthcare, Life Science, Milan, Italy). About 1000 RU of human recombinant hnRNP A2 (Origene Technologies, Rockville, USA) were immobilized on Serie S sensor chip CM5 by amine coupling chemistry. Immobilization was performed in HEPES-NaCl running buffer (HEPES pH 7.4 10mM, NaCl 150mM, EDTA 3mM). Flow cell 1 was blank immobilized to permit reference subtraction. Binding analysis of LTR-II+III+IV, LTR-II+III+IV M4+5 and LTR-II+III+IV Random sequences was performed at a flow rate of 25μl/min, with contact time and dissociation time of 120s in HEPES-KCl buffer (HEPES pH 7.4 10mM, KCl 150mM, EDTA 3mM). Oligonucleotides folding into G4 structures was performed in HEPES-KCl buffer after heat denaturation at 95°C for 5min and gradual cooling at room temperature. Sensograms were obtained in the concentration range of 31.25nM–2μM. After each oligonucleotide injection the chip surface was regenerated with NaCl 2.5M solution. All sensograms were corrected by double reference subtraction of blank flow cell response and buffer injection response. Data were fitted to a global 1:1 binding model using BIAevaluation software (GE Healthcare).
Oligonucleotides were diluted to 0.1μM in lithium cacodylate buffer (10mM, pH 7.4) and KCl (indicated in figure legends) heat denatured for 5min at 95°C, and folded in G-quadruplex structure at room temperature for 16h. Samples were incubated alone, with hnRNP A2 or bovine serum albumin (BSA, negative control) and subsequently fluorescence intensity was monitored from 30°C to 95°C (1°C/min) in a LightCycler II (Roche, Milan, Italy) by observing 6-carboxyfluorescein (6FAM) emission. FRET efficiency (E) was calculated as the total fluorescence intensity of the donor in the absence (ID) and presence of the acceptor (IDA), by using E=1−(IDA/ID). ID and IDA values were obtained on a LS 55 Fluorescence spectrometer (Perkin Elmer, Waltham, MA, USA) setting the excitation wavelength at 480nm and recording the emission from 500 to 650nm. The dual-labelled oligonucleotide was converted into the corresponding duplex, in which the fluorophores are at a distance (R) for which FRET is ~0. R was calculated from FRET efficiency values as , where R0 (Förster distance) is the distance at which energy transfer is 50% of the maximum value. Between FAM and TAMRA fluorophores, R0 is assumed to be 5026. F-test (F) and the probability (P) values were calculated using R statistical environment (v. 3.3.2)31. A conventional alpha=0.05 was considered to evaluate the test significance.
Taq polymerase stop assay was carried out as previously described18,22. Briefly, the 5′-end labelled primer was annealed to its template (Table S1) in lithium cacodylate buffer in the presence or absence of KCl (50–100mM) and by heating at 95°C for 5min and gradually cooling to room temperature. Where specified, samples were incubated with 29 ng of human recombinant hnRNP A2 (Origene Technologies, Rockville, USA) at 37°C for 15min. Primer extension was conducted with 2 U of AmpliTaq Gold DNA polymerase (Applied Biosystem, Carlsbad, California, USA) at 37°C for 30min. Reactions were stopped by ethanol precipitation, primer extension products were separated on a 15% denaturing gel, and finally visualized by phosphorimaging (Typhoon FLA 9000).
DNA oligonucleotides were diluted to a final concentration (4μM) in lithium cacodylate buffer (10mM, pH 7.4) and KCl 100mM. Samples were annealed by heating at 95°C for 5min and gradually cooled to room temperature overnight. CD spectra were recorded on a Chirascan-Plus (Applied Photophysisics, Leatherhead, UK) equipped with a Peltier temperature controller using a quartz cell of 5 mm optical path length, over a wavelength range of 230–320nm. For the determination of Tm, spectra were recorded over a temperature range of 20–90°C, with temperature increase of 5°C. The reported spectra are baseline-corrected for signal contributions due to the buffer. Observed ellipticities were converted to mean residue ellipticity (θ)=deg×cm2×dmol−1 (mol ellip). Tm values were calculated according to the van’t Hoff equation, applied for a two-state transition from a folded to unfolded state, assuming that the heat capacity of the folded and unfolded states are equal52.
Immunoblot analysis was performed on cell protein extracts obtained in RIPA Buffer (20mM Tris-HCl pH 7.5; 150mM NaCl, 1mM EDTA, 1% NP-40, 1% sodium deoxycholate, 1mM Na3VO4, 1x protease inhibitors). Protein concentrations were quantified using the Pierce® BCA Protein Assay Kit (Thermo Scientific, Rockford, IL, USA). Each sample was electrophoresed on 10% SDS-PAGE and transferred to a nitrocellulose blotting membrane (Amersham TM Protan TM, GE Healtcare Life science, Milan, Italy) by using trans-blot SD semi-dry transfer cell (Bio-Rad Laboratories, Milan, Italy). The membranes were blocked with 2.5% skim milk in PBST (0.05% Tween 20 in PBS). Membranes were incubated with the respective primary antibody directed against hnRNP A2/B1 (mouse monoclonal; Santa Cruz Biotechnology, Dallas, TX, USA), alpha-tubulin (mouse monoclonal; Sigma-Aldrich, Milan, Italy). After three washes in PBST, membranes were incubated with ECL Plex Goat-α-Mouse IgG-Cy5 (GE Healthcare Life sciences, Milan, Italy). Images were captured on the Typhoon FLA 9000.
Gene-specific pooled siRNA trilencer targeting human hnRNP A2/B1 and a scrambled negative control duplex were purchased from Origene (human hnRNP A2/B1 Trilencer-27 Human siRNA, OriGene Technologies, Rockville, MD, USA). 293T cells or TZM-bl reporter cells were transfected with increasing concentrations of siRNA (1, 2, 4 and 8nM for 293T and 1, 5, 10nM for TZM-bl cells) and scrambled siRNA by using Lipofectamine RNAiMAX (Invitrogen, Thermo Fisher Scientific, Waltham, MA, USA) following the manufacturer’s instructions. Only for experiments in 293T cells, pLTR luciferase plasmids (pGL4.10-LTRwt or pGL4.10-LTR-M4+5) were transfected 24h later by using Lipofectamine 3000 (Invitrogen, Thermo Fisher Scientific, Waltham, MA, USA). Luciferase activity was measured using the britelite plus Reporter Gene Assay System (PerkinElmer Inc., Milan, Italy) at a Victor X2 multilabel plate reader (PerkinElmer Inc., Milan, Italy), according to the manufacturer’s instructions. Cells were lysed in 1% Triton-X100-PBS and protein concentration was determined by BCA assay (Thermo Scientific Pierce, Monza, Italy). Luciferase signals were subsequently normalized to total protein content, according to the manufacturer’s protocol (http://ita.promega.com/~/pdf/resources/pubhub/cellnotes/normalizing-genetic-reporter-assays/). Each assay was performed in duplicate and each set of experiments was repeated at least three times.
The MTT (3-(4,5-dimethylthiazol 2-yl)-2,5-diphenyltetrazolium bromide, Sigma Aldrich, Milan Italy) assay was performed to assess cell viability on silenced cells. 293T cells (6×103) were plated in 96-well plates and incubated for 24h. Following siRNA transfection (from 1nM to 8nM), cells were incubated for an additional 48h. Control cells (transfected in absence of siRNA) were treated in the exact same conditions. Cell survival was evaluated by MTT assay: 10μL of freshly dissolved solution of MTT (5mg/mL in PBS) were added to each well, and after 4h of incubation, MTT crystals were solubilized in solubilization solution (10% sodium dodecyl sulphate (SDS) and 0.01M HCl). After overnight incubation at 37°C, absorbance was read at 540nm. Data were expressed as mean values of at least two individual experiments conducted in triplicate. The percentage of cell survival was calculated as follows: cell survival=(Awell−Ablank)/(Acontrol−Ablank)×100, where blank denotes the medium without cells.
How to cite this article: Scalabrin, M. et al. The cellular protein hnRNP A2/B1 enhances HIV-1 transcription by unfolding LTR promoter G-quadruplexes. Sci. Rep. 7, 45244; doi: 10.1038/srep45244 (2017).
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This work was supported by the Bill and Melinda Gates Foundation (GCE grant numbers OPP1035881, OPP1097238); the European Research Council (ERC Consolidator grant 615879); and the Italian Ministry of University and Research (FIRB-Ideas RBID082ATK) to SNR. Funding for open access charge: Bill and Melinda Gates Foundation.
The authors declare no competing financial interests.
Author Contributions M.S. performed the mass spectrometry analysis and protein identification; I.F. provided silencing, reporter and viability data in cells, E.R. performed the FRET analysis, R.P. performed the Taq polymerase stop assays and silencing in TZM-bl cells, E.T. performed the pull-down assay and western blot, S.L. provided the SPR data, M.T. performed CD analysis, G.P. commented on the manuscript, S.N.R. conceived of the work and wrote the manuscript. All authors analyzed the data and reviewed the manuscript.