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Tumor-derived exosomes have been shown to induce various immunomodulatory effects. However, the underlying signaling pathways are poorly understood. Here, we analyzed the effects of ex vivo-derived exosomes on monocytic cell differentiation/activation using THP-1 cells as model. We isolated exosomes from various body fluids such as amniotic fluid, liver cirrhosis ascites, and malignant ascites of ovarian cancer patients. We observed that exosomes were internalized by THP-1 cells and induced the production of IL-1β, TNF-α, and IL-6. Analysis of the signaling pathways revealed a fast triggering of NFκB and a delayed activation of STAT3. Pharmacologic and antibody-blocking experiments showed that the initial production of IL-6 was instrumental for subsequent activation of STAT3. Importantly, triggering of cell signaling was not a unique property of tumor exosomes but was also observed with exosomes of noncancerous origin. Exosomal signaling was TLR-dependent as the knockdown of Toll-like receptor 2 (TLR2) and TLR4 blocked NFκB and STAT3 activation. Similar results were obtained with TLR-neutralizing antibodies. Exosomes also triggered the release of cytokines from mouse bone marrow-derived dendritic cells or macrophages. This process was MyD88-dependent, further supporting a role of TLR signaling. Our results suggest that exosomes trigger TLR-dependent signaling pathways in monocytic precursor cells but possibly also in other immune cells. This process could be important for the induction of immunosuppressive mechanisms during cancer progression and inflammatory diseases.
Exosomes are small membrane vesicles released from many different cell types in the body such as erythrocytes, platelets, lymphocytes, dendritic cells (DCs)3 and tumor cells (1–3). Exosomes are formed by invagination and budding from the limiting membrane of late endosomes (4, 5). It is believed that they accumulate in cytosolic multivesicular bodies from where they are released by fusion with the plasma membrane in a Rab-dependent manner (4–6). This process is very active in proliferating cells, such as cancer cells (7). Depending on the cellular origin, the protein composition of exosomes can differ from that of the plasma membrane. Exosomal proteins include MHC molecules, tetraspanins, adhesion molecules, and metalloproteinases (1, 2, 8). In addition to functional proteins, exosomes carry mRNAs as well as miRNAs (9–12). Exosomes can be engulfed by other cells, and it was proposed that this transfer of protein and RNAs from one to another cell might represent a novel mechanism of intercellular communication (4, 9, 13).
Exosomes play an important role in modulating immune responses (14, 15). When derived from dendritic cells, they bear MHC proteins and co-stimulatory molecules (2, 16). These vesicles are effective in stimulating antigen-specific T cell responses in vitro and in vivo. In contrast, exosomes from tumor cells or those released from the fetus during pregnancy can suppress immune responses (15, 17–22). It was found that tumor-derived exosomes can directly inhibit natural killer cell or T cell function (19, 23), block dendritic cell maturation (24), induce MDSCs (15, 25, 26), or augment the activity of regulatory T cells (17, 27). Cancer-derived microvesicles can modify the surrounding stroma and promote the process of fibroblast differentiation into myofibroblasts (28). They foster the interplay of stroma cells with breast tumor cells (29). These effects support tumor growth and suppress innate and adaptive immune responses.
It is presently unknown which signal pathways exosomes trigger in recipient cells to induce an immunosuppressive phenotype. Recent work has shown that the induction of MDSCs from precursors involved TLR signaling and STAT3 activation (25, 30). Another study has shown that miRNAs in cancer-released exosomes can reach and bind TLRs and induce prometastatic inflammatory responses (31). However, it is unclear whether these properties are unique to cancer-derived exosomes or are an intrinsic feature of all exosomes.
In this paper we have addressed the questions of whether exosomes can modulate the biological functions of monocytic cells and which signaling pathways are activated by exosomes. We show that microvesicles are taken up by human monocytic THP-1 cells and stimulate cytokine release and NFκB/STAT3 activation. We also show that the initiation of this signaling is TLR-dependent and can be elicited not only by tumor-derived exosomes.
Antibodies to human CD24 (SWA11), ADAM10 (11G2), and CD9 (TS9) have been described (32–34). The mAbs to HSP70, Annexin-1, Tsg101, and CD9 were from BD Transduction. The antibodies to GAPDH or p65 were from Santa Cruz Biotechnologies. The antibodies against STAT3, p-STAT3 (Y705) and phospho-p65 (S536) were obtained from Cell Signaling. Neutralizing antibodies to IL-6 and IL-6 receptor were a kind gift from Prof. Stefan Rose-John, University of Kiel, Germany. TLR2 and TLR4 neutralizing antibodies and TLR agonists (LPS, PAM3CSK4, and R848) were obtained from Invivogen. Fluorochrome-conjugated mAbs for FACS analysis of TLR2 (Biolegend 121805) or TLR4 (E Bioscience 17-9917) were used at a dilution of 1:200. Lentiviral shRNA particles (each five shRNA clones) for stable knockdown of TLR2 (NM_003264.2) or TLR4 (NM_003266.2) as well as control particles (shEGFP) were obtained from Sigma-Aldrich. Phorbol 12-myristate 13-acetate (PMA) was from Sigma-Aldrich. Parthenolide (IκB kinase inhibitor), P6 (pyridone 6/JAK2 inhibitor), and AG490 (JAK1 inhibitor) were from Calbiochem.
Analysis of patient-derived material was under the approval of the ethics commission of the University of Heidelberg. Human amniotic fluid was collected for routine amniocentesis and analyzed after removal of cells. Exosomes were isolated by differential centrifugation as described (32). The purification of exosomes from the ascites of liver cirrhosis patients was described before (12, 32). All purified exosomes were dissolved in PBS, and the protein concentration was determined using a Bradford protein quantification kit (Bio-Rad). BSA was used as standard. NanoSight analysis was carried out by courtesy of the company (NanoSight, Amesbury, Wiltshire, UK).
THP-1 cells were seeded into 15-ml conical tubes (THP-1, 2 × 106 cells/tube). Depending on the experiment, cells were treated with body fluid exosomes (40–200 ng/μl) in a total volume of 500 μl of serum-free RPMI 1640 medium for different periods of time (30 min to 48 h). After treatment, lysates were analyzed by Western blotting or RT-PCR. In case of co-incubation of cells with exosomes and antibodies, antibodies were used at a concentration of 1–3 μg/ml unless otherwise indicated. Treatment of cells with heat-inactivated or enzymatically digested exosomes were performed accordingly (40 ng/μl exosomes/2 × 106 cells in a total volume of 500 μl of serum-free medium). Co-treatment of cells with exosomes and inhibitors was performed with 20 μg (40 ng/μl) of exosomes in the presence of either 10 μm parthenolide, 2 μm pyridone 6 (P6), or 10 μm AG490, respectively.
Purified exosomes were heat-inactivated by incubation at 95 °C for 5–10 min on a heating block. For enzymatic digestion, 100–170 μg of exosomes was digested in the presence of 10 μg/ml DNase I, 10 μg/ml RNase A, or 10 μg/ml protease K, respectively, for 1.5 h at 37 °C. To inhibit protease K after digestion, the digestion mix was supplied with 100 μm PMSF.
For the transduction of THP-1 monocytes with lentiviral particles, 2 × 105 cells were pelleted in 15-ml conical tubes (1000 × g, 5 min). Five different shTLR2- and shTLR4-viral particle clones as well as one shEGFP control clone were used to transduce cells. Cells were spinoculated (1000 × g, 1 h at 22 °C) in the presence of particles at a respective multiplicity of infection of 1. Cells undergoing spinoculation in the absence of virus further served as cytotoxicity control under selection conditions. After centrifugation and aspiration of virus-containing supernatant, cells were resuspended in growth medium (DMEM, 10% FCS) and transferred to 12-well plates. Transduced cells were grown under standard cell culture conditions for another 72 h before being placed in selection medium (0.6 μg/ml puromycin in growth medium). Expansion under selective conditions was continued for 14 days.
FACS analysis of isolated vesicles was done after adsorbing of isolated vesicles to 4 nm (surfactant-free) aldehyde-sulfate latex beads (Interfacial Dynamics, Portland, OR) as described (34). The staining of beads or cultivated cells with mAbs and phycoerythrin-conjugated secondary antibodies has been described (32, 34). Stained beads or cells were analyzed with a FACScan using Cellquest software (BD Biosciences).
THP-1 cells (1.0 × 105) were incubated for 24 h in the presence of malignant ascites (AS) exosomes (50 μg/ml) in a 96-well format. Plastic-adherent cells were washed with PBS and incubated for 90 min at 37 °C with 10 μl of 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) solution (5 mg/ml) in 100 μl of RPMI 1640 medium. After incubation, the plate was centrifuged, and supernatant was discarded. Per well, 100 μl of dimethyl sulfoxide was added and incubated for 10 min at room temperature. The amount of released formazan was measured at 570 nm.
THP-1 cells (2.5 × 105) were seeded in 100 μl of RPMI 1640 medium + 50 μg/ml exosomes in the upper chamber of a Boyden chamber (pore size 5 μm). The lower chamber was filled with 400 μl of RPMI 1640 medium. After a 24-h incubation, migrated cells were detached from the bottom side of the membrane by incubation with trypsin/EDTA and combined with the cell containing medium of the lower chamber. Migrated cells were quantified with CASY® Cell Analyzer systems.
Bone marrow cells from 8–12-week-old C57BL/6 WT or C57BL/6-MyD88−/− mice were collected from femur bone marrow elutions. DCs were matured by incubation with supernatant from the X63 plasmocytoma cell line producing murine GM-CSF in RPMI 1640 medium, 10% FCS, 1% penicillin/streptomycin, 0.05 mm β-mercaptoethanol for 8 days. Macrophages were differentiated in DMEM supplemented with 30% L929 supernatant, 10% FCS, and 1% penicillin/streptomycin for 7 days. DCs and macrophages (each 2 × 105/well) were stimulated with 8 μg of amniotic fluid (AF) exosomes or various TLR agonists (1 μg/ml) in a 96-well (DCs) or 48-well (macrophages) format for 16 h. Cell-free supernatants were used for detection of indicated cytokines using specific ELISAs (BD Biosciences).
RT-PCR was performed as described before (35). Briefly, total RNA from cells was isolated and transcribed using the ReverseAid H Minus First Strand cDNA Synthesis kit (Fermentas, St. Leon-Rot, Germany), purified on Microspin G-50 columns (GE Healthcare) and quantified by a NanoDrop Spectrophotometer (ND-2000; Thermo Scientific). Primers were designed using the IDT primer quest program and were produced by MWG (Ebersberg, Germany). β-Actin was used as an internal standard. The sequences of primers are available on request.
Cell pellets were solubilized in lysis buffer (250 mm NaCl, 50 mm HEPES, 0.5% Nonidet P-40, 10% glycerol, 2 mm EDTA, 10 mm NaF, 1 mm sodium orthovanadate, 1 mm PMSF, 10 mg/ml each leupeptin and aprotinin) for 30 min on ice. Lysates were cleared by centrifugation and boiled with reducing or nonreducing SDS loading buffer. Samples were separated on SDS-polyacrylamide gels and transferred to Immobilon membranes using semidry blotting. After blocking with 4% BSA in Tween 20/TBS, membranes were probed with primary antibodies followed by horseradish peroxidase-conjugated secondary antibody and ECL detection (Amersham Biosciences).
Cytokines in cell culture supernatants were analyzed using a Bio-Plex Pro Human Cytokine 27-plex assay (Bio-Rad).
Data are presented as the mean ± S.E. Student's unpaired t test was used to evaluate the difference between groups. p < 0.05 was considered statistically significant.
We previously isolated exosomes by differential centrifugation from human AS, serum, and urine (11, 12). A similar protocol was used to collect exosomes from AF. An average of 7.21 μg/ml (range 1.6–13 μg/ml, n = 64) of protein was recovered per AF sample, which is comparable with the yield reported for AS. Density gradient centrifugation and transmission EM analysis for AS and liver cirrhosis (LC) exosomes were performed previously (12). Nanosight analysis showed a size distribution of 100–300 nm for both types of exosomes (Fig. 1A). Biochemical analysis revealed that AS and AF exosomes were positive for the established exosomal marker proteins HSP70, Annexin-1, and LAMP1 as well as the ESCRT component Tsg101 (Fig. 1B).
Exosomes are released from cells by fusion of multivesicular bodies with the plasma membrane and have an orientation of antigens facing outside (1, 5). We confirmed the orientation of antigens by FACS analysis after immobilization of the vesicles on latex beads. We observed stronger staining with antibodies to CD24 and ADAM10 and weaker staining for CD9 and β1-integrin. These proteins were previously described to occur in exosomes (1, 12). The uptake of CFSE-labeled exosomes was investigated in the human monocytic precursor cell line THP-1. As detected by FACS analysis, the uptake proceeded in a time-dependent fashion and was augmented when THP-1 cells were pretreated with PMA before the assay (Fig. 1C). The degree of uptake was variable and patient-dependent. Fluorescent microscopy showed that labeled exosomes localized inside of the cells (Fig. 1D).
Upon differentiation into macrophages THP-1 cells become plastic-adherent. We examined whether the incubation with exosomes affected the adhesion and motility of THP-1 cells. When tested 24 h after exosome exposure, THP-1 cells showed enhanced adhesiveness to plastic and augmented migration in Boyden chamber assays (Fig. 1E). Although to a different extent, this was observed with exosomes from several patients.
We next analyzed THP-1 cells for changes in gene expression after exosome exposure. We found that exosomes induced a dose-dependent up-regulation of IL-1β as measured by RT-PCR (Fig. 1F). Enhanced release of IL-1β was detected by ELISA (Fig. 1F). The induction was again dose-dependent and abolished by boiling exosomes before addition to the cells (Fig. 1G). In human blood monocytes tumor-derived exosomes trigger the release of cytokines, including IL-6, TNF-α, and TGF-β (26). We therefore extended the analysis of cytokines released by THP-1 cells. To find out whether also non-tumor-derived exosomes could trigger cytokine release, we compared AS-derived with AF-derived exosomes. By RT-PCR (Fig. 2A) and Bio-Plex analysis (Fig. 2B) we found strong induction of cytokines such as IL-6, IL-1β, TNF-α, IL-23a, and IL-8. Importantly, at the dose tested (40 μg/ml) both types of exosomes enhanced production and secretion of cytokines in a comparable fashion.
Previous work had shown that ex vitro-derived exosomes from tumor cell lines could trigger NFκB signaling (31, 36) and activate STAT3 (25, 30). In THP-1 cells we investigated the signaling events triggered by exosomes. We observed a rapid activation of NFκB as detected by phosphorylation of the p65 subunit that peaked at 30–120 min after exosome exposure (Fig. 2C). STAT3 activation was delayed and became only obvious after 6–12 h (Fig. 2C). The kinetic of activation was similar for AF-, AS-, and LC-derived exosomes. Additionally, exosomes from in vitro cultured A125 lung cancer cells showed comparable activation of NFκB and STAT3. Phosphorylation of STAT3 after 12 h was also seen when cells were stimulated for control with LPS but not with BSA (Fig. 2D). Rapid activation of STAT3 (3–10 min) was shown when THP-1 cells were treated with IL-6-enriched supernatant (Fig. 2E). This clearly demonstrated that exosomal activation of STAT3 was temporally different from classical activation by IL-6.
Interestingly, for LC exosomes an early STAT3 phosphorylation after 30 min was also noticed (Fig. 2C). Of note, when body fluid-derived exosomes were examined for the content of cytokines, LC exosomes carried IL-6. Most likely this reflected their origin from an inflammatory background. We concluded that the property to stimulate NFκB and late STAT3 activation in THP-1 cells is not a unique property of tumor-derived exosomes but is shared by exosomes from other sources.
STAT3 phosphorylation is classically induced by the activation of the IL-6/JAK2/STAT3 pathway (37). We argued that IL-6 produced in the first wave of NFκB activation would subsequently trigger STAT3 phosphorylation in an autrocrine/paracrine fashion. In support of this, we found that STAT3 activation was blocked in the presence of the specific NFκB inhibitor parthenolide and the JAK2-specific inhibitor P6 but not by the JAK1 inhibitor AG490 (Fig. 3A).
Strikingly, the treatment with parthenolide abolished the induction of cytokine genes by exosomes as determined for IL-6, TNF-α, and IL-1β by RT-PCR (Fig. 3B). Treatment with P6 also reduced the level of IL-6 in agreement with the notion that IL-6 is also a STAT3-dependent gene (38). These findings suggested that a cytokine was the likely mediator between the initial NFκB and delayed STAT3 activation and that the observed signaling events were linked to the induction of cytokine genes.
To further solidify the important role of IL-6, we employed neutralizing mAbs to IL-6 and IL-6 receptor. When THP-1 cells were stimulated with exosomes in the presence of anti-IL-6 or anti-IL-6 receptor antibodies no phosphorylation of STAT3 was observed (Fig. 3C).
To find out which determinant on exosomes was responsible for signal initiation, we treated exosomes with DNase, RNase, or proteinase K before exposure to THP-1 cells. Only boiling at 95 °C (Fig. 4A) or proteinase K treatment (Fig. 4B) completely abolished NFκB and STAT3 activation. In contrast, boiling of LPS did not destroy the ability to trigger NFκB and STAT3 activation (Fig. 4A). Importantly, the enzymes alone did not trigger activation of THP-1 cells (Fig. 4C). Collectively, these findings together with those presented in Fig. 1G emphasized that an LPS contamination was unlikely to be the source of triggering. Our data rather suggested that a protein determinant associated with exosomes is responsible for the induction of p65 phosphorylation.
It is known that TLRs can activate the NFκB pathway. Indeed, we noticed that the effects of exosomes on cell signaling were similar to TLR agonists. This prompted us to study more closely the role of TLRs in exosome-mediated signaling. THP-1 cells expressed TLR2 and TLR4 but were negative for TLR7 and TLR8 as detected by RT-PCR (Fig. 5A). In agreement with this expression profile, strong stimulation was observed with the TLR1/2 agonist PAM3CSK4 (P3C4) and LPS, a known ligand to TLR4 (Fig. 5B). In contrast, no stimulation was seen with the TLR7/8 ligand R848 (Fig. 5B).
To find out which TLRs were involved in exosome signaling, we stably silenced TLR2 and TLR4 expression by lentiviral-transduced shRNA. As determined by FACS analysis, the THP-1/shTLR2-transduced cells showed significantly diminished expression of TLR2 (67% decrease) compared with the control cells (shEGFP) (Fig. 5C). A similar reduction of TLR4 was seen in THP-1/shTLR4 (52% decrease) (Fig. 5C). The knockdown was specific for the respective TLRs as confirmed by RT-PCR analysis (Fig. 5C). Activation of p65 and STAT3 was also reduced in THP-1/shTLR2 and THP-1/shTLR4 cells (Fig. 5C) The stimulation of knockdown cells with the TLR agonists P3C4 and LPS, respectively, was reduced by >95% for IL-6 and 30–50% for IL-1β (Fig. 5D).
Importantly, the exosome signaling was also impaired. In TLR4 knock-out cells the production of IL-6 and IL-1β was strongly decreased compared with the control cells (Fig. 5E). In THP-1/shTLR2 cells the exosomal stimulation was slightly less affected but also reached significance at the 48-h time point (Fig. 5E). In addition, both types of knockdown cells secreted less IL-1β, IL-6, INF-γ, TNF-α, and IL-23a which was mostly apparent after 48 h (Fig. 5F).
Finally, we investigated whether functional blocking antibodies to TLR2 or TLR4 could inhibit exosome-mediated signaling. Indeed, we observed that antibodies to TLR2 and TLR4 could partially inhibit the exosome-mediated phosphorylation of STAT3 and induction of IL-1β and IL-6 mRNA and that this effect was additive when both antibodies were combined (Fig. 6A). Collectively, these data implicate that TLR2 and TLR4 are relevant for exosome-mediated signaling.
To further demonstrate the importance of TLRs we made use of knock-out mice deficient for the TLR downstream signaling-component MyD88. We stimulated mouse DCs and macrophages with human exosomes. Cytokine release revealed induction of TNF-α and IL-12 in DCs and macrophages of wild-type mice. Importantly, in mice deficient for MyD88 no activation was observed (Fig. 6B). These findings further supported a role for TLRs in exosome-mediated signaling.
Membrane vesicles in the form of exosomes are released from normal and cancer cells. However, significantly enhanced levels of exosomes are found in the sera or AS of cancer patients, and the amount is often correlated with the stage of the disease (12, 39, 40). There is evidence that exosomes released by the tumor can suppress the immune system of the patient and prepare niches for metastatic spread (41). In the present report we have asked how exosomes can interact and stimulate immune cells using monocytic THP-1 cells as a model. We find that (i) exosomes are internalized by THP-1 cells and stimulate the expression and secretion of cytokines; (ii) this feature is not restricted to cancer-derived exosomes but is also observed with exosomes from nontumorous sources; (iii) for cytokine release the signaling via the NFκB and STAT3 pathways is instrumental; (iv) TLR2 and TLR4 on the cell surface and a proteinase-sensitive determinant on exosomes are responsible for signal initiation. Our results suggest that exosomes have inherent signaling capacity that could be important for the induction of immunosuppression.
Previous studies showed immunosuppressive effects of tumor-derived exosomes from cell culture supernatants. Such exosomes are derived from cells that have undergone multiple passages ex vivo in the absence of any selective pressure from the immune system. Contrary to exosomes from cell culture, we assumed that exosomes from body fluid are more likely to reflect the in vivo situation. Thus, in the current study, a main goal was to deepen the understanding of immune cell stimulation by ex vivo-derived exosomes. Indeed, microvesicles isolated from various body fluids including those from AS, LC ascites, urine, and amniotic fluid have been previously characterized in our laboratory and identified as exosomes (12, 32, 33, 42). Surprisingly, we found in the present study that exposure of such exosomes to THP-1 cells could trigger NFκB and STAT3 activation and cytokine release. The secretion of proinflammatory mediators could be induced with AS exosomes coming from a tumor background. Intriguingly, however, exosomes from non-cancer-associated body fluids such as AF or LC exosomes were at least equally capable of triggering gene expression and secretion of proinflammatory mediators. In the course of this study, we purified and tested exosomes from many different ascites and amniotic fluid samples and found that the potency to activate THP-1 cells could differ between exosomal batches. This could be because exosome number was estimated by means of protein concentrations in exosome preparations. Protein concentration, in turn, might be a poor indicator of exosome number. However, this could also reflect differences in the composition of exosomes. Nevertheless, all tested sources of exosomes were generally potent and reliable activators of THP-1 cells. Thus, we hypothesized that exosomes from different body fluids, malignant or nonmalignant, carry common determinant(s) that enable them to activate THP-1 cells.
We found that STAT3 was not directly activated by exosomes. Pharmacological and antibody-mediated inhibition experiments indicated that the initial activation of NFκB leading to the production of IL-6 was required for subsequent STAT3 activation in a paracrine/autocrine fashion. Similar conclusions were reported previously in the study of Chalmin et al. (25). We also provide evidence that activation of the NFκB and STAT3 pathways were necessary for the induction of cytokine genes. Collectively, these data provide novel insights into the signaling potential of exosomes.
We also show that in THP-1 cells the TLRs are key receptors for exosome-mediated signaling. This is based on the following findings: (i) the stable knockdown of TLR2 or TLR4 led to a partial reduction of cytokine gene induction and release; (ii) antibodies to TLR2 and TLR4 alone could block in part the phosphorylation of STAT3 and subsequent induction of IL-1β and IL-6 transcription, but the effect was strongest when both antibodies were used in combination; (iii) human exosomes could trigger secretion of cytokines in mouse DCs and macrophages, but this was abolished in cells deficient for MyD88, an adaptor protein required for TLR signaling. Our results confirm and extend previous work demonstrating a functional role of TLR2 (25, 30). For the first time we also show an involvement of TLR4. Previous studies have focused mostly on mouse systems and tissue culture-derived exosomes, and a role of TLR4 was not investigated. Meanwhile Fabbri et al. reported that miRNAs in exosomes can trigger the endosomal TLR7/8 leading to cytokine secretion (31). Due to the absence of these receptors in THP-1 cells we were unable to investigate this. Our data do not exclude the possibility that in addition to TLRs other molecules can serve as exosomal receptors on monocytic or other immune cells.
An important question is which determinants on exosomes trigger TLRs and cytokine production. Previous studies have reported conflicting results. Xiang et al. proposed that exosomes isolated from in vivo grown breast adenocarcinomas were able to induce expansion of MDSCs via a mechanism dependent on the exosomal presence of prostaglandin E2 (43). Chalmin et al. used cell-culture derived exosomes and found that activation of MDSCs was dependent on the presence of HSP72 on exosomes whereas no exosomal prostaglandin E2 was found in their study (25). Using body fluid-derived exosomes we observed that the stimulating potential was destroyed by proteinase K but not with DNase or RNase treatment, supporting the notion that signals come from proteins. These determinant(s) need to be further characterized. It should be borne in mind that beside HSPs other alarmins including HMGB1 or S100 proteins were shown to be potentially secreted on exosomes (44–46).
A limitation of our current study is due to the THP-1 cells used as model system being a transformed cell line. Additional studies with primary monocytes are clearly needed. In part such studies have been already performed. Work from the Rivoltini laboratory has demonstrated that CD14+ monocytes isolated from healthy donors and differentiated with IL-4 and GM-CSF in the presence of tumor-derived microvesicles turned into HLA-DR−/low cells, retaining CD14 expression and failed to up-regulate co-stimulatory molecules, such as CD80 and CD86. The phenotypic changes were paralleled by a significant release of different cytokines, including IL-6, TNF-α, and TGF-β (47). Thus, cytokine production by exosomes has also been seen in nontransformed cells, but the exact signaling pathways were not elucidated. Although our data lay the ground for a better understanding of signaling pathways engaged by exosomes in monocytic cells, we can presently not explain how tumor-derived exosomes induce immunosuppression under physiological conditions. Perhaps a critical factor in the process is the amount of exosomes and the presence of other immunosuppressive factors in the tumor microenvironment. Increased amounts of exosomes might surpass a certain threshold of activation. As illustrated in Fig. 7, it is our hypothesis that cancer-released exosomes initiate a signaling cascade involving cytokines such as IL-6 and activation of STAT3 in tumor cells and immune cells. This milieu could alter tumor-infiltrating immune cells in a way favoring immunosuppression and the escape of the tumor from immunosurveillance (14).
We thank Natalie Erbe-Hoffmann for excellent technical assistance and Prof. Alexander Dalpke, University of Heidelberg, and Dr. Kai Doberstein for continuous support and discussions.
*This work was supported by Deutsche Krebshilfe Project 109745 and by the Deutsches Krebsforschungszentrum/Tumorzentrum Collaborative Program (to P. A. and F. M.).
3The abbreviations used are: