- Open Access
Human T-cell leukemia virus type-I Tax induces the expression of CD83 on T cells
Retrovirology volume 12, Article number: 56 (2015)
CD83, a cell surface glycoprotein that is stably expressed on mature dendritic cells, can be transiently induced on other hematopoietic cell lineages upon cell activation. In contrast to the membrane form of CD83, soluble CD83 appears to be immunosuppressive. In an analysis of the phenotype of leukemic CD4+ T cells from patients with adult T-cell leukemia (ATL), we found that a number of primary CD4+ T cells became positive for cell surface CD83 after short-term culture, and that most of these CD83+ CD4+ T cells were positive for human T-cell leukemia virus type-I (HTLV-I) Tax (Tax1). We hypothesized that Tax1 is involved in the induction of CD83.
We found that CD83 was expressed selectively on Tax1-expressing human CD4+ T cells in short-term cultured peripheral blood mononuclear cells (PBMCs) isolated from HTLV-I+ donors, including ATL patients and HTLV-I carriers. HTLV-I-infected T cell lines expressing Tax1 also expressed cell surface CD83 and released soluble CD83. CD83 can be expressed in the JPX-9 cell line by cadmium-mediated Tax1 induction and in Jurkat cells or PBMCs by Tax1 introduction via infection with a recombinant adenovirus carrying the Tax1 gene. The CD83 promoter was activated by Tax1 in an NF-κB-dependent manner. Based on a previous report showing soluble CD83-mediated prostaglandin E2 (PGE2) production from human monocytes in vitro, we tested if PGE2 affected HTLV-I propagation, and found that PGE2 strongly stimulated expression of Tax1 and viral structural molecules.
Our results suggest that HTLV-I induces CD83 expression on T cells via Tax1 -mediated NF-κB activation, which may promote HTLV-I infection in vivo.
CD83 is a 40–50-kDa cell surface glycoprotein that is a member of the sialic-acid-binding immunoglobulin-like lectin family, and is a marker of mature dendritic cells (DCs) in humans and mice . In contrast to mature DCs, which stably express high levels of CD83 , previous studies suggest that CD83 is transiently expressed on other hematopoietic cell lineages and tissues, including activated T cells and B cells [1, 3–5], macrophages , neutrophils , and NK cells  in vitro, and hematopoietic tissues  and skin Langerhans cells  in vivo.
Two isoforms of CD83, a membrane-bound form (mCD83) and a soluble form (sCD83) have been identified; sCD83 is likely a result of shedding the mCD83 isoform . mCD83 critically functions not only in the development of CD4+ T cells in the thymus , but also in T cell activation  and the longevity of B and CD4+ T cells . In contrast, sCD83 functions as a suppressor of T cell activation . A recent study has shown that sCD83 suppresses the differentiation of DCs from monocytes . Elevated levels of plasma sCD83 have been demonstrated in patients with hematological malignancies . Kreiser et al. showed that the in vitro culture of mCD83-expressing fresh regulatory T cells in mice leads to the release of sCD83 . Although the molecular mechanisms by which sCD83 mediates T cell suppression are not fully understood, human sCD83 may mediate its inhibitory effect on T cell responses via prostaglandin E2 (PGE2) produced by monocytes .
Human T-cell leukemia virus type-I (HTLV-I) is a human retrovirus that is etiologically associated with adult T-cell leukemia (ATL)  and HTLV-I-associated myelopathy/tropical spastic paraparesis (HAM/TSP) [17, 18]. The majority of HTLV-I carriers remain asymptomatic throughout their lives, and approximately 5% of HTLV-I-infected individuals develop either ATL or HAM/TSP after prolonged latency periods . HTLV-I encodes Tax (Tax1), which activates viral transcription and promotes mechanisms that are critical for cell growth and division, leading to viral replication . The effects of Tax1 on cells include potent NF-κB activation, cell cycle perturbation, and cell transformation . In addition to Tax1, the basic leucine zipper of HTLV-I (HBZ) has been proposed to play an important role in the oncogenesis of ATL by HTLV-I . However, the precise mechanisms by which HTLV-I infection leads to disease development remain poorly understood.
HTLV-I is transmitted through contact with body fluids containing infected cells; common examples include mother-to-child transmission . It is difficult to detect HTLV-I-antigen-expressing cells in fresh PBMCs from HTLV-I infected individuals. When PBMCs are cultured for a short period of time, some T cells begin to produce HTLV-I antigens  followed by spontaneous immortalization of cells in cultures containing interleukin-2 (IL-2) . CD8+ cytotoxic T lymphocyte (CTL)  and neutralizing antibody  responses specific to HTLV-I play important roles in controlling HTLV-I propagation in HTLV-I carriers. It is noteworthy that not only ATL patients, but also healthy HTLV-I carriers are prone to immunodeficiency [27–31]. Curiously, monocytes from HTLV-I+ donors exhibit a deficiency in the ability to differentiate into mature DCs in vitro, and cultured immature DCs show low levels of CD83 expression in association with poor T cell stimulation .
In an analysis of phenotypes of PBMCs from ATL patients and HTLV-I carriers living in Okinawa prefecture, Japan, where ATL is prevalent, we detected high levels of CD83 expression in primary CD4+ T cells from PBMCs of HTLV-I+ donors after short-term in vitro culture. Surprisingly, most of these CD83+ cells from HTLV-I+ donors were positive for Tax1. Herein, we show that Tax1 is responsible for the induction of CD83 on T cells, and discuss its possible role(s) in HTLV-I infection.
CD83 expression on Tax1+ cells
In a phenotypic analysis of fresh and in vitro cultured PBMCs from ATL patients in Okinawa, we noticed that short-term cultivation induced CD83 expression in a subpopulation of CD4+ T cells in PBMCs (Figure 1a, b). Interestingly, a majority of the CD83-positive CD4+ T cells exhibited detectable levels of intracellular Tax1 expression. The Tax1 expression in cultured PBMCs from ATL patients was confirmed by a western blot analysis with our anti-Tax1 monoclonal antibody (mAb) (Lt-4) (Additional file 1: Figure S1). Similar acquisition of CD83 on Tax1+ cells was observed in cultured PBMCs from HTLV-I carriers and HAM/TSP patients (data not shown). In contrast, only low levels of CD83 expression were observed in normal PBMCs cultured in vitro without mitogen. Cultures with mitogen exhibited increased CD83 expression in a small population of CD3- PBMCs (Figure 1c), which were predominantly CD19+ (data not shown), indicating that those CD83+ cells were B lymphocytes.
We next examined CD83 expression with a panel of HTLV-I+ T cell lines. All of the Tax1+ cell lines tested, including the IL-2-independent T cell lines (MT-2, HUT102, and MT-1) and IL-2-dependent T cell lines derived from an ATL patient (ATL-026), a HAM/TSP patient (ILT-M1), or a healthy donor whose T cells were transformed in vitro by HTLV-I (YT/cM1), were positive for CD83 (Figure 2a). It is noteworthy that an ATL patient-derived HTLV-I-infected T cell line that lacks Tax1 expression (TL-Om1) was negative for CD83 expression. In addition, the HTLV-I+ rat T cell line W7TM-1, and the human HTLV-II+ T cell line Ton1 were also positive for rat and human CD83, respectively (Figure 2b). The HTLV-I-negative human T cell lines CEM, Molt-4, and Jurkat and the HIV-1-producing Molt4/IIIB were negative for CD83 (data not shown). CD83 expression thus appeared to parallel the expression of Tax1. These results suggest a relationship between CD83 and Tax1 expression.
The expression of CD83 in HTLV-I+ cells was confirmed by western blot analyses using our laboratory-derived mAb (rat IgG, clone W83#8). As shown in Figure 3, the apparent molecular weight (MW) of the major CD83 molecule in HTLV-I+ HUT102 cells was 48 kDa, which was comparable to that of ectopically expressed CD83 on 293T cells (293T/CD83). Since the protein core of CD83 has an estimated MW of 21 kDa and is heavily glycosylated , we inferred that the other CD83-specific bands ranging between 40 and 70 kDa may be CD83 isoforms with different levels of glycosylation.
We next examined the production of sCD83 by HTLV-I+ T cells. Levels of CD83 in cell lysates and culture supernatants were quantitated using a commercial enzyme-linked immunosorbent assay (ELISA) kit. All Tax1+ T cell lines tested produced readily detectable levels of sCD83 in culture supernatants (Figure 4). The relative levels of sCD83 were estimated at approximately 10–20% of CD83 levels associated with cells. Since plasma sCD83 is elevated in some patients with chronic lymphocytic leukemia , we attempted to determine the levels of sCD83 in plasma samples obtained from acute ATL patients. Out of 11 ATL samples, only one showed a significantly higher sCD83 level (>1,000 pg/ml) than normal (<20 pg/ml) (data not shown).
CD83 induction by Tax1
The potential ability of Tax1 to induce CD83 expression was examined using the Tax1-inducible human T cell line JPX-9. Incubation with CdCl2, which is required for Tax1 expression, induced apparent cell surface CD83 expression on JPX-9 cells (Figure 5a). Importantly, CD83 expression was predominantly restricted to Tax1+ cells. The majority of Tax1+ cells also expressed OX40, a representative protein that is also induced by Tax1 on T cells .
To confirm the Tax1-mediated CD83 expression, CD83 mRNA levels were quantitated by real-time PCR using peripheral blood mononuclear cells (PBMCs) and Jurkat cells following infection with recombinant adenovirus encoding Tax1 (Figure 5b). CD83 mRNA levels were significantly elevated in both PBMCs and Jurkat cells. These results are consistent with the concept that Tax1 induces cell surface expression of CD83, and suggest that the effect of Tax1 on CD83 expression occurs at the transcriptional level. Taken together, these data strongly imply that CD83 is a member of the HTLV-I Tax-inducible protein family.
Enrichment of live Tax1+ and Tax1− cells by cell sorting
It may be noteworthy that the triple-positive (Tax1+ CD83+ OX40+) phenotype was found in primary CD4+ T cells from an ATL patient (Figure 6). Generally, IL-2-dependent HTLV-I-infected T cell lines derived from HTLV-I+ donors consist of HTLV-I antigen-positive and -negative cells, especially during the early culture stage with low passages. Flow cytometry-based cell sorting cannot separate live Tax1+ cells from live Tax1− cells owing to intracellular localization of Tax1. Based on the present finding that most Tax1+ cells expressed both CD83 and OX40, we attempted to sort live Tax1+ and Tax1− cells. An IL-2 dependent HTLV-I+ T cell line (OKH4) from a HAM/TSP patient was stained with anti-OX40 and anti-CD83 mAbs, and subjected to cell sorting. CD83+ OX40+ sorting efficiently enriched the Tax1+ cell population (Figure 7). Similar enrichment of Tax1+ cells was obtained with three IL-2-dependent HTLV-I+ T cell lines (data not shown). This strategy would be useful for further studies on Tax1 function in pHTLV-I-infected primary T cells.
Tax1-responsive elements in the CD83 promoter
To gain insight into the molecular mechanism of Tax1-dependent induction of CD83, the CD83 promoter was examined by reporter assays. Jurkat cells were transfected with a luciferase reporter plasmid, pCD83(-537)Luc, carrying the isolated wild-type CD83 promoter along with the Tax1 expression plasmid. The CD83 promoter was profoundly activated by Tax1 (Figure 8a). In efforts to localize the CD83 promoter sequences with biological activity, reporter assays were performed using a series of 5′ deletion constructs of the CD83 promoter. These studies showed that pCD83(-101)Luc retained activity to promote transcription in response to Tax1, similar to pCD83(-537)Luc, while pCD83(-29)Luc did not respond to Tax1 (Figure 8a). The observations indicate that a Tax1-responsive element(s) in the CD83 promoter is located in the region between −101 and −30. A computer search identified two possible NF-κB binding sites between the −101 to −30 region of the CD83 promoter (Figure 8b). We next investigated the potential role of those NF-κB binding sites in Tax1-mediated activation of CD83 gene transcription. This objective was achieved using substitution mutations that were introduced to either each of the possible NF-κB binding sites or to both sites (Figure 8c). Upon expression of Tax1, each single mutant showed an approximate 50% decrease in promoter activity compared with the wild-type CD83 promoter (Figure 8d). Little, if any, response to Tax1 was observed for the mutant pCD83(-537 κBmt1/2)Luc carrying mutations at both sites (Figure 8d).
The Tax1-mediated upregulation of CD83 expression via NF-κB activation was verified by reporter assays on a series of Tax1 mutants. All Tax1 mutants except for TaxM22, which lacks the NF-κB activation function, facilitated CD83 promoter activity (Figure 9). TaxM22 did not show significant induction of luciferase activity from pCD83(-537)Luc. Collectively, these results demonstrate that the two NF-κB binding sites are critical for the induction of CD83 expression in response to Tax1. HTLV-II Tax2B also upregulated CD83 promoter activity, consistent with cell surface expression of CD83 by the HTLV-II+ cells (Figure 2b).
Stimulation of Tax1 expression and HTLV-I production by PGE2
sCD83 has been reported to stimulate PGE2 production from human monocytes and to suppress T cell activation in vitro . We thus tested the effects of PGE2 on HTLV-I expression in an ATL-derived HTLV-I+ T cell line (ATL-056). PGE2 induced marked expression of Tax1 (Figure 10a). In addition, we observed an increase in expression of the viral envelope protein gp46 and release of viral core protein p24 to the culture supernatants (Figure 10a). Figure 10b shows that PGE2 treatment increased the syncytium-inducing activity of ATL-056 cells, suggesting that PGE2 enhances cell-to-cell infectivity of HTLV-I.
In the present study, we showed for the first time that CD83 is expressed by Tax1+ cells in primary cultures of CD4+ T cells and HTLV-I- or HTLV-II-infected CD4+ or CD8+ T cell lines. Fresh ATL leukemic T cells express CD2, CD5, CD4, CD25, CD29, CD40RO, CD194, T cell receptor α/β, and HLA-DR with diminished CD3 expression , but they do not express Tax1. Cultures of primary CD4+ T cells from HTLV-I+ donors and HTLV-I+ T cell lines express additional cell surface markers including the T cell activation markers (CD40, CD80, and CD86), TNF/TNFR family members (GITR, 4-1BB, 4-1BBL, OX40, and OX40L), the chemokine receptors/interleukin receptors (CCR7 and CCR8), and a number of cell adhesion molecules, such as CD58/LFA3, CD54/ICAM-1, and VCAM-1. Some of those molecules are induced by Tax1 , and the present study adds CD83 to the list of members of the HTLV-I and -II Tax-inducible protein family.
Tax1 is a transcriptional modulator that lacks the ability to directly bind to DNA elements; rather, it modifies cellular transcription factor activity, in particular via NF-κB, CREB, and SRF. Among these factors, NF-κB attenuated by Tax1 is critically involved in immortalization and transformation. The present study demonstrates that Tax1-mediated induction of CD83 is absolutely dependent on the NF-κB pathway, similar to that reported for OX40  and OX40L . It has been reported that the Epstein-Barr virus latent membrane protein 1 (LMP1), which is known to activate the NF-κB pathway, also induces CD83 expression in human B lymphocytes, in which an NF-κB binding site in the CD83 promoter is responsive for LMP1-mediated activation . Our present study revealed that another NF-κB binding site in the CD83 promoter was responsive to NF-κB activated by Tax1 in human T cells. It is of interest that the activation of NF-κB is insufficient for CD83 induction since a TL-Om1 cell line that contains a single copy of the HTLV-I provirus, but does not express Tax1, was negative for CD83 expression (Figure 2), while NF-κB in TL-Om1 is constitutively activated . Thus, Tax1 expression may determine the promoter binding specificity and/or transcriptional regulation of NF-κB target genes such as CD83, OX40, and OX40L. Further studies are required to clarify the additional requirements for CD83 induction by Tax1.
The potential for CD83 induction by Tax1 in HTLV-I infections that leads to leukemogenesis or the onset of a neurological disorder, remains unknown. So far, CD83 modulation has been linked to virus escape from the T cell immune system. For example, human cytomegalovirus (HCMV) infection of DCs has been shown to inhibit T cell stimulation via release of sCD83 , and human herpes simplex virus (HSV) infection of mature DCs has been shown to downregulate the cell surface expression of CD83 by degradation of CD83 via the cellular proteasome . Because the expression of either Tax1 or CD83 on CD4+ T cells is difficult to detect and monitor in the peripheral blood, even in acute ATL patients (Figure 1), Tax1-induced CD83 seems to be indirectly associated with the onset of ATL or HAM/TSP. However, observations of the steady presence of strong CTL and high levels of antibody responses specific for HTLV-I antigens in HTLV-I+-infected individuals indicate the persistent production of HTLV-I in vivo. In addition, an immunodeficiency was found in ATL patients or healthy carriers [27–31], and the inability of monocytes from HTLV-I+ donors to differentiate into mature DCs has been reported . Integration of these results may provide some clues regarding the roles of CD83 in HTLV-I infection. First, Bates et al. recently reported that the homotypic interaction of mCD83 via cell-to-cell contact inhibits pro-inflammatory responses (including IL-12 production) induced by DCs ; accordingly, mCD83 induced on HTLV-I+ CD4+ T cells may interact with mCD83 on immuno-stimulated DCs in vivo and suppress IL-12 production, presumably resulting in inhibition of anti-HTLV-I Th1 responses. Second, sCD83 released from Tax1+ CD4+ T cells may interact with monocytes and stimulate the production of the pleotropic bioregulator PEG2. PEG2 has been reported to enhance HTLV-I gag p19 production from PBMC cultures of HTLV-I carriers  and to stimulate HTLV-I LTR in combination with CD3/CD28 activation in human T cell lines . Consistent with these observations, we showed in the present study that PGE2 alone enhanced the expression of HTLV-I Tax1 and HTLV-I-mediated cell fusion (Figure 10). Therefore, it can be speculated that sCD83-induced PGE2 from monocytes stimulates HTLV-I production and the expansion of HTLV-I+ CD4+ T cells via the induction of Tax1 expression in a paracrine manner. However, our preliminary experiments failed to show that soluble recombinant CD83 actually enhances HTLV-I infection in vitro via production of PGE2 from primary monocytes. Further studies to test our hypotheses, including the link between T-cell activation by mCD83 and enhanced HTLV-I infection, are in progress.
Since normal human T cells express low to undetectable levels of CD83, high expression of both CD83 and OX40 on a single CD4+ T cell is a good marker of intracellular Tax1 expression. The sorting method for cells directly stained with anti-Tax antibody does not enable enrichment for live Tax1+ cells due to the required fixation and permeabilization of cells . Thus, the present findings could provide a useful method for the enrichment of live Tax1+ T cells, as shown in Figure 7, and presumably will contribute to further studies on Tax1 function in the development and maintenance of HTLV-I-related diseases.
The present study documents the potential role of HTLV-I Tax in the induction of CD83 cell surface expression and release of sCD83 in an NF-κB-dependent manner in human CD4+ T cells in vitro, which may indirectly suppress immune responses and promote HTLV-I infection in vivo in terms of virus transmission to new target cells and expansion and/or survival of infected T cell clones.
The medium used throughout was RPMI 1640 medium (Sigma-Aldrich. Inc., St. Louis, MO, USA) supplemented with 10% fetal calf serum (FCS), 100 U/ml penicillin and 100 µg/ml streptomycin (hereinafter called RPMI medium). Mouse monoclonal antibodies (mAbs) specific for HTLV-I Tax (clone Lt-4), OX40 (clone B-7B5), and KLH (IgG3, clone KLH-3, Tanaka et al., unpublished) were purified in our laboratory from ascites fluids of CB.17-SCID mice carrying the appropriate hybridomas. The ascites fluid samples were subjected to ammonium sulfate precipitation followed by gel filtration with Superdex G-200 (GE Healthcare, Tokyo, Japan). mAbs were labeled with either fluorescein isothiocyanate (FITC) or HiLyte Fluor™ 647 using commercial labeling kits (Dojindo, Kumamoto, Japan) according to the manufacturer’s instructions. FITC-, PE- or PE-Cy7-labeled mouse mAbs against human CD3, CD4, CD8, CD14, CD19, CD56, and CD83 (clone H15e), and FITC-labeled goat anti-rat IgG, donkey anti-rabbit IgG, and HRP-labeled goat anti-rat IgG antibodies were purchased from BioLegend (Tokyo, Japan). Rabbit polyclonal IgG anti-rat CD83 antibody was obtained from Sino Biological (Beijing, China). Prostaglandin E2 (PGE2) was purchased from Sigma-Aldrich. Inc., (St. Louis, MO, USA).
The protocols for the use of human PBMCs and animals were approved by the Human IRB and the Institutional Animal Care and Use Committee (IACUC) on clinical and animal research of the University of the Ryukyus and Tokyo Medical and Dental University prior to the initiation of the study. All human samples were collected after obtaining written informed consent according to the Declaration of Helsinki. PBMCs were isolated from heparinized blood by a standard density gradient centrifugation . HTLV-I-producing T cell lines were IL-2-independent T cell lines (MT-1, MT-2, and HUT102), IL-2-dependent CD4+ and CD8+ T cell lines derived from various HTLV-I+ donors (ATL patients, HAM/TSP patients, or asymptomatic HTLV-I carriers), and CD4+ T cell lines derived from normal PBMCs established by co-cultivation with mitomycin C-treated HTLV-I-producing cells . The TL-Om1 cell line is an ATL-patient-derived IL-2-independent HTLV-I-infected T cell line not expressing the Tax antigen . The HTLV-I+ rat T cell line was W7TM-1 . The HTLV-I-negative human T cell lines were Jurkat, CEM, Molt-4, Molt-4/IIIB, and Jurkat-derived JPX-9, in which Tax1 can be induced by cultivation in the presence of 10 μM CdCl2 . The HTLV-II+ human T cell line was Ton1 . Cell lines were cultured in RPMI medium in the presence of 20 U/ml recombinant human IL-2, if necessary. For select experiments, human PBMCs were stimulated with 10 μg/ml phytohemagglutinin (PHA) (Wako, Japan) or immobilized anti-CD3 and anti-CD28 mAbs (BioLegend). Derivatives of 293T cells expressing human CD83 (293T/CD83) and its vector control (293T/CT) were established in our laboratory by transfection of 293T cells with human CD83 vector (pCAGIPuro/CD83) and empty vector (pCAGIPuro), respectively.
Syncytium induction assay was performed using a combination of ILT-M1 and Jurkat cells as described previously .
Generation of a new anti-CD83 mAb
Hybridomas producing mAbs against human CD83 were generated from spleen cells of WKA rats immunized with recombinant human CD83-Fc fusion protein (R&D Systems, Inc., Cosmo Bio, Tokyo, Japan) by cell fusion with the SP2/0 myeloma cell line utilizing the Sendai virus cell fusion kit (GenomeONE, Cosmo Bio), and screened by ELISA using CD83-Fc-coated plates (0.1 μg/ml per well) and goat anti-rat IgG-HRP antibody (BioLegend). mAbs were further selected based on their abilities to stain CD83 expressed on 293T/CD83 cells but not 293T/CT cells. Western blots were performed as reported previously . The anti-CD83 mAbs established by this screening included clones W83#4 and W83#8, both of which were rat IgG2b and applicable for flow cytometry. The clone W83#4, but not W83#8, competed in a binding assay with a commercially available mouse anti-human CD83 mAb clone H15e. The clone W83#8, but not W83#4 or H15e, was applicable for western blot analysis (data not shown).
Flow cytometry (FCM), cell sorting, and ELISA
Phenotypic analyses of cells were carried out using polychromatic flow cytometry (FCM) as reported previously . Briefly, live cells were Fc-blocked with 2 mg/ml pooled normal human IgG in FACS buffer [PBS containing 0.2% bovine serum albumin (BSA) and 0.1% sodium azide] for 10 min on ice, followed by incubation with fluorescent-dye labeled mAbs for 30 min. After washing with FACS buffer, the cells were fixed in 4% paraformaldehyde (PFA) in PBS for 5 min at room temperature followed by permeabilization and washing in FACS buffer containing 0.5% saponin and 1% BSA (Sigma). An aliquot of the stained cells was incubated with 0.1 μg/ml HiLyte Fluor™ 647-labeled anti-Tax1 antibody (clone Lt-4) for 30 min. Negative control cells were stained with HiLyte Fluor™ 647-labeled Lt-4 in the presence of 100 μg/ml unlabeled Lt-4. These cells were analyzed using a FACSCalibur (BD, Franklin Lakes, NJ, USA) and data obtained were analyzed using the Cell Quest software (BD).
To sort CD83 and OX40 double-positive and double-negative cell populations, IL-2-dependent T cell lines established from HTLV-I+ donors were stained with PE-Cy7-labeled anti-CD83 (clone H15e) and PE-labeled anti-OX40 (clone B-7B5) mAbs, and then subjected to sorting using a cell sorter SH800Z (Sony, Tokyo, Japan) equipped with appropriate filters for multi-color analysis in a dual semiconductor laser (488)/(639 nm) system.
sCD83 in culture supernatants and cell lysates were quantitated using a commercial ELISA kit (MyBiosource, San Diego, CA, USA). HTLV-I p24 production into the culture supernatants was determined by our in-house formulated ELISA .
Expression plasmids for Tax1 (pMT-2Tax), Tax2B (pHβAP-r1-neo Tax2B), and Tax1 mutants were derived using the pHβAP-r-1-neo system with the human β-actin promoter [49, 50]. Tax1 mutants lacking the ability to activate NF-κB (TaxM22), CREB (Taxd3), and SRF (Tax703) in T cells have been described previously . The luciferase reporter plasmids for the NF-κB site (pκB-Luc), CREB binding site (pLTR-Luc), and CArG box (pCArG-Luc) have been described elsewhere [51–53]. The CD83 reporter plasmid [pCD83(-537)Luc] was generated by insertion of a 578-bp fragment (−537 to +41 from the transcription start site ) amplified from human genomic DNA by PCR using forward (5′-acgctagccatggaaatctaacgcgccttt-3′) and reverse (5′-gtaagcttggctggagcgctgcgccgctgc-3′) primer pairs. The insert was cloned into the NheI and HindIII sites of the pGL3-basic vector. A series of 5′ deletion mutants of the human CD83 promoter was generated by PCR and inserted into pGL3-basic, yielding pCD83(-285)Luc, pCD83(-146)Luc, pCD83(-101)Luc, and pCD83(-29)Luc. The substitution mutants of the two possible NF-κB binding sites in the CD83 promoter were generated by PCR using the mutant primers, yielding pCD83(-537 κBmt1)Luc, pCD83(-537 κBmt2)Luc, and pCD83(-537 κBmt1/2)Luc with mutations at the NF-κB1 site, NF-κB2 site, and both sites, respectively (see Figure 8c, d).
Infection with adenoviruses
Recombinant adenovirus for Tax1 (Ad-Tax1)  was generated with the ViraPower adenoviral expression system with the CAG promoter according to the supplier’s instructions. PBMCs and Jurkat cells were infected at an MOI of 100 or 10 plaque forming units (PFU)/cell, respectively, as previously described [56, 57].
Total RNA was extracted using Isogen (Nippon Gene Co. Ltd., Tokyo, Japan) according to the supplier’s protocol. First-strand cDNA was synthesized using the first-strand cDNA synthesis kit for reverse transcription-PCR (AMV; Roche, Tokyo, Japan). Quantification of CD83 gene expression was performed utilizing the forward (5′-gcgacgccggaggtgaaggtg-3′) and reverse (5′-tccccgagttgcagctggtagtgt-3′) primer pair using a LightCycler (Roche). The 18S rRNA primers were obtained from TaKaRa (Shiga, Japan).
Jurkat cells were transfected with Tax expression plasmids along with reporter plasmids by the DEAE-dextran method described previously . Cell lysates were prepared for determination of luciferase activity using the luciferase assay system (Promega, Tokyo, Japan) according to the manufacture’s recommendations. Normalization of luciferase activity was performed against the cell lysate protein concentration that was measured by the DC Protein Assay Kit (Bio-Rad, Tokyo, Japan). The assays were repeated at least three times and the mean ± SE values are shown.
A paired t-test was performed for statistical analysis. P-values of less than 0.05 were considered significant.
human T-cell leukemia virus type-I
a transactivator from the X-gene region of HTLV-I
adult T-cell leukemia
peripheral blood mononuclear cells
SDS-polyacrylamide gel electrophoresis
Keyhole limpet hemocyanin
Zhou LJ, Schwarting R, Smith HM, Tedder TF (1992) A novel cell-surface molecule expressed by human interdigitating reticulum cells, Langerhans cells, and activated lymphocytes is a new member of the Ig superfamily. J Immunol 149:735–742
Cao W, Lee SH, Lu J (2005) CD83 is preformed inside monocytes, macrophages and dendritic cells, but it is only stably expressed on activated dendritic cells. Biochem J 385:85–93
Wolenski M, Cramer SO, Ehrlich S, Steeg C, Grossschupff G, Tenner-Racz K et al (2003) Expression of CD83 in the murine immune system. Med Microbiol Immunol 192:189–192
Prazma CM, Yazawa N, Fujimoto Y, Fujimoto M, Tedder TF (2007) CD83 expression is a sensitive marker of activation required for B cell and CD4+ T cell longevity in vivo. J Immunol 179:4550–4562
Reinwald S, Wiethe C, Westendorf AM, Breloer M, Probst-Kepper M, Fleischer B et al (2008) CD83 expression in CD4+ T cells modulates inflammation and autoimmunity. J Immunol 180:5890–5897
Yamashiro S, Wang JM, Yang D, Gong WH, Kamohara H, Yoshimura T (2000) Expression of CCR6 and CD83 by cytokine-activated human neutrophils. Blood 96:3958–3963
Mailliard RB, Alber SM, Shen H, Watkins SC, Kirkwood JM, Herberman RB et al (2005) IL-18-induced CD83+ CCR7+ NK helper cells. J Exp Med 202:941–953
Fujimoto Y, Tu L, Miller AS, Bock C, Fujimoto M, Doyle C et al (2002) CD83 expression influences CD4+ T cell development in the thymus. Cell 108:755–767
Hock BD, Kato M, McKenzie JL, Hart DN (2001) A soluble form of CD83 is released from activated dendritic cells and B lymphocytes, and is detectable in normal human sera. Int Immunol 13:959–967
Aerts-Toegaert C, Heirman C, Tuyaerts S, Corthals J, Aerts JL, Bonehill A et al (2007) CD83 expression on dendritic cells and T cells: correlation with effective immune responses. Eur J Immunol 37:686–695
Lechmann M, Krooshoop DJ, Dudziak D, Kremmer E, Kuhnt C, Figdor CG et al (2001) The extracellular domain of CD83 inhibits dendritic cell-mediated T cell stimulation and binds to a ligand on dendritic cells. J Exp Med 194:1813–1821
Lin H, Liang S, Zhong Z, Wen J, Li W, Wang L et al (2014) Soluble CD83 inhibits human monocyte differentiation into dendritic cells in vitro. Cell Immunol 292:25–31
Hock BD, Fernyhough LJ, Gough SM, Steinkasserer A, Cox AG, McKenzie JL (2009) Release and clinical significance of soluble CD83 in chronic lymphocytic leukemia. Leuk Res 33:1089–1095
Kreiser S, Eckhardt J, Kuhnt C, Stein M, Krzyzak L, Seitz C et al (2015) Murine CD83-positive T cells mediate suppressor functions in vitro and in vivo. Immunobiology 220:270–279
Chen L, Zhu Y, Zhang G, Gao C, Zhong W, Zhang X (2011) CD83-stimulated monocytes suppress T-cell immune responses through production of prostaglandin E2. Proc Natl Acad Sci USA 108:18778–18783
Hinuma Y, Nagata K, Hanaoka M, Nakai M, Matsumoto T, Kinoshita KI (1981) Adult T-cell leukemia: antigen in an ATL cell line and detection of antibodies to the antigen in human sera. Proc Natl Acad Sci USA 78:6476–6480
Gessain A, Barin F, Vernant JC, Gout O, Maurs L, Calender A et al (1985) Antibodies to human T-lymphotropic virus type-I in patients with tropical spastic paraparesis. Lancet 2:407–410
Osame M, Matsumoto M, Usuku K, Izumo S, Ijichi N, Amitani H et al (1987) Chronic progressive myelopathy associated with elevated antibodies to human T-lymphotropic virus type I and adult T-cell leukemialike cells. Ann Neurol 21:117–122
Ishitsuka K, Tamura K (2014) Human T-cell leukaemia virus type I and adult T-cell leukaemia-lymphoma. Lancet Oncol 15:e517–e526
Yoshida M (2010) Molecular approach to human leukemia: isolation and characterization of the first human retrovirus HTLV-1 and its impact on tumorigenesis in adult T-cell leukemia. Proc Jpn Acad Ser B Phys Biol Sci 86:117–130
Romanelli MG, Diani E, Bergamo E, Casoli C, Ciminale V, Bex F et al (2013) Highlights on distinctive structural and functional properties of HTLV Tax proteins. Front Microbiol 4:271
Matsuoka M, Yasunaga J (2013) Human T-cell leukemia virus type 1: replication, proliferation and propagation by Tax and HTLV-1 bZIP factor. Curr Opin Virol 3:684–691
Hinuma Y, Gotoh Y, Sugamura K, Nagata K, Goto T, Nakai M et al (1982) A retrovirus associated with human adult T-cell leukemia: in vitro activation. Gan 73:341–344
Gotoh YI, Sugamura K, Hinuma Y (1982) Healthy carriers of a human retrovirus, adult T-cell leukemia virus (ATLV): demonstration by clonal culture of ATLV-carrying T cells from peripheral blood. Proc Natl Acad Sci USA 79:4780–4782
Bangham CR (2009) CTL quality and the control of human retroviral infections. Eur J Immunol 39:1700–1712
Tanaka Y, Takahashi Y, Tanaka R, Kodama A, Fujii H, Hasegawa A et al (2014) Elimination of human T cell leukemia virus type-1-infected cells by neutralizing and antibody-dependent cellular cytotoxicity-inducing antibodies against human t cell leukemia virus type-1 envelope gp46. AIDS Res Hum Retroviruses 30:542–552
Murphy EL, Glynn SA, Fridey J, Smith JW, Sacher RA, Nass CC et al (1999) Increased incidence of infectious diseases during prospective follow-up of human T-lymphotropic virus type II- and I-infected blood donors. Retrovirus Epidemiology Donor Study. Arch Intern Med 159:1485–1491
Yamazato Y, Miyazato A, Kawakami K, Yara S, Kaneshima H, Saito A (2003) High expression of p40(tax) and pro-inflammatory cytokines and chemokines in the lungs of human T-lymphotropic virus type 1-related bronchopulmonary disorders. Chest 124:2283–2292
Santos SB, Porto AF, Muniz AL, de Jesus AR, Magalhaes E, Melo A et al (2004) Exacerbated inflammatory cellular immune response characteristics of HAM/TSP is observed in a large proportion of HTLV-I asymptomatic carriers. BMC Infect Dis 4:7
Funai N, Shimamoto Y, Yoshida S, Nagai Y, Nakazato S, Kohashi O (1996) Differences in immune functions between human T-lymphotropic virus type I carriers and patients with adult T-cell leukemia/lymphoma. Clin Immunol Immunopathol 80:325–332
Yasunaga J, Sakai T, Nosaka K, Etoh K, Tamiya S, Koga S et al (2001) Impaired production of naive T lymphocytes in human T-cell leukemia virus type I-infected individuals: its implications in the immunodeficient state. Blood 97:3177–3183
Nascimento CR, Lima MA, de Andrada Serpa MJ, Espindola O, Leite AC, Echevarria-Lima J (2011) Monocytes from HTLV-1-infected patients are unable to fully mature into dendritic cells. Blood 117:489–499
Hock BD, Haring LF, Steinkasserer A, Taylor KG, Patton WN, McKenzie JL (2004) The soluble form of CD83 is present at elevated levels in a number of hematological malignancies. Leuk Res 28:237–241
Higashimura N, Takasawa N, Tanaka Y, Nakamura M, Sugamura K (1996) Induction of OX40, a receptor of gp34, on T cells by trans-acting transcriptional activator, Tax, of human T-cell leukemia virus type I. Jpn J Cancer Res 87:227–231
Kress AK, Grassmann R, Fleckenstein B (2011) Cell surface markers in HTLV-1 pathogenesis. Viruses 3:1439–1459
Ohtani K, Tsujimoto A, Tsukahara T, Numata N, Miura S, Sugamura K et al (1998) Molecular mechanisms of promoter regulation of the gp34 gene that is trans-activated by an oncoprotein Tax of human T cell leukemia virus type I. J Biol Chem 273:14119–14129
Dudziak D, Kieser A, Dirmeier U, Nimmerjahn F, Berchtold S, Steinkasserer A et al (2003) Latent membrane protein 1 of Epstein-Barr virus induces CD83 by the NF-kappaB signaling pathway. J Virol 77:8290–8298
Mori N, Fujii M, Ikeda S, Yamada Y, Tomonaga M, Ballard DW et al (1999) Constitutive activation of NF-kappaB in primary adult T-cell leukemia cells. Blood 93:2360–2368
Senechal B, Boruchov AM, Reagan JL, Hart DN, Young JW (2004) Infection of mature monocyte-derived dendritic cells with human cytomegalovirus inhibits stimulation of T-cell proliferation via the release of soluble CD83. Blood 103:4207–4215
Kummer M, Turza NM, Muhl-Zurbes P, Lechmann M, Boutell C, Coffin RS et al (2007) Herpes simplex virus type 1 induces CD83 degradation in mature dendritic cells with immediate-early kinetics via the cellular proteasome. J Virol 81:6326–6338
Bates JM, Flanagan K, Mo L, Ota N, Ding J, Ho S et al (2015) Dendritic cell CD83 homotypic interactions regulate inflammation and promote mucosal homeostasis. Mucosal Immunol 8:414–428
Moriuchi M, Inoue H, Moriuchi H (2001) Reciprocal interactions between human T-lymphotropic virus type 1 and prostaglandins: implications for viral transmission. J Virol 75:192–198
Dumais N, Pare ME, Mercier S, Bounou S, Marriot SJ, Barbeau B et al (2003) T-cell receptor/CD28 engagement when combined with prostaglandin E2 treatment leads to potent activation of human T-cell leukemia virus type 1. J Virol 77:11170–11179
Melamed A, Laydon DJ, Gillet NA, Tanaka Y, Taylor GP, Bangham CR (2013) Genome-wide determinants of proviral targeting, clonal abundance and expression in natural HTLV-1 infection. PLoS Pathog 9:e1003271
Tanaka Y, Tozawa H, Koyanagi Y, Shida H (1990) Recognition of human T cell leukemia virus type I (HTLV-I) gag and pX gene products by MHC-restricted cytotoxic T lymphocytes induced in rats against syngeneic HTLV-I-infected cells. J Immunol 144:4202–4211
Miura S, Ohtani K, Numata N, Niki M, Ohbo K, Ina Y et al (1991) Molecular cloning and characterization of a novel glycoprotein, gp34, that is specifically induced by the human T-cell leukemia virus type I transactivator p40tax. Mol Cell Biol 11:1313–1325
Ootsuyama Y, Shimotohno K, Miwa M, Oroszlan S, Sugimura T (1985) Myristylation of gag protein in human T-cell leukemia virus type-I and type-II. Jpn J Cancer Res 76:1132–1135
Tanaka R, Yoshida A, Murakami T, Baba E, Lichtenfeld J, Omori T et al (2001) Unique monoclonal antibody recognizing the third extracellular loop of CXCR4 induces lymphocyte agglutination and enhances human immunodeficiency virus type 1-mediated syncytium formation and productive infection. J Virol 75:11534–11543
Gunning P, Leavitt J, Muscat G, Ng SY, Kedes L (1987) A human beta-actin expression vector system directs high-level accumulation of antisense transcripts. Proc Natl Acad Sci USA 84:4831–4835
Matsumoto K, Shibata H, Fujisawa JI, Inoue H, Hakura A, Tsukahara T et al (1997) Human T-cell leukemia virus type 1 Tax protein transforms rat fibroblasts via two distinct pathways. J Virol 71:4445–4451
Akagi T, Ono H, Nyunoya H, Shimotohno K (1997) Characterization of peripheral blood T-lymphocytes transduced with HTLV-I Tax mutants with different trans-activating phenotypes. Oncogene 14:2071–2078
Hirai H, Suzuki T, Fujisawa J, Inoue J, Yoshida M (1994) Tax protein of human T-cell leukemia virus type I binds to the ankyrin motifs of inhibitory factor kappa B and induces nuclear translocation of transcription factor NF-kappa B proteins for transcriptional activation. Proc Natl Acad Sci USA 91:3584–3588
Fujisawa J, Toita M, Yoshida M (1989) A unique enhancer element for the trans activator (p40tax) of human T-cell leukemia virus type I that is distinct from cyclic AMP- and 12-O-tetradecanoylphorbol-13-acetate-responsive elements. J Virol 63:3234–3239
Kozlow EJ, Wilson GL, Fox CH, Kehrl JH (1993) Subtractive cDNA cloning of a novel member of the Ig gene superfamily expressed at high levels in activated B lymphocytes. Blood 81:454–461
Mizuguchi M, Asao H, Hara T, Higuchi M, Fujii M, Nakamura M (2009) Transcriptional activation of the interleukin-21 gene and its receptor gene by human T-cell leukemia virus type 1 Tax in human T-cells. J Biol Chem 284:25501–25511
Hirai H, Fujisawa J, Suzuki T, Ueda K, Muramatsu M, Tsuboi A et al (1992) Transcriptional activator Tax of HTLV-1 binds to the NF-kappa B precursor p105. Oncogene 7:1737–1742
Ohtani K, Iwanaga R, Arai M, Huang Y, Matsumura Y, Nakamura M (2000) Cell type-specific E2F activation and cell cycle progression induced by the oncogene product Tax of human T-cell leukemia virus type I. J Biol Chem 275:11154–11163
Ohtani K, Nakamura M, Saito S, Noda T, Ito Y, Sugamura K et al (1987) Identification of two distinct elements in the long terminal repeat of HTLV-I responsible for maximum gene expression. EMBO J 6:389–395
YTan conceived of the study, participated in its design and coordination, carried out the FCM assays, and drafted the manuscript. MM and MN carried out molecular studies, YTak established the CD83-expressing cell line and ATL T cell lines, HF carried out the cell sorting, RT produced, purified, and labeled mAbs, confirmed their specificities, and made in-house EILSA kits, TF and TT collected blood samples from HTLV-I+ patients, and AAA participated in the design of the study and helped to draft the manuscript. All authors read and approved the final manuscript.
We thank Prof. M. Fujii at Niigata University for providing Ton1 cells. This work was supported by grants from the Ministry of Education, Culture, Sports, Science, and Technology and the Ministry of Health, Labor, and Welfare of Japan, and Okinawa prefecture.
Compliance with ethical guidelines
Competing interests The authors declare that they have no competing interests.
Figure S1. Western blot analysis of Tax1 expression in PBMCs from an ATL patient (ATL #5) before or after a one-day culture. Cell lysates were subjected to SDS-PAGE on a 5–20% gel, and blotted onto PVDF membranes. The membranes were incubated with either mouse anti-human Tax1 mAb (clone Lt-4) or IgG3 isotype control mAb (anti-KLH), followed by treatment with HRP-labeled goat anti-mouse IgG antibody.
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Tanaka, Y., Mizuguchi, M., Takahashi, Y. et al. Human T-cell leukemia virus type-I Tax induces the expression of CD83 on T cells. Retrovirology 12, 56 (2015). https://doi.org/10.1186/s12977-015-0185-1