Interaction and uptake of exosomes by ovarian cancer cells
BMC Cancer volume 11, Article number: 108 (2011)
Exosomes consist of membrane vesicles that are secreted by several cell types, including tumors and have been found in biological fluids. Exosomes interact with other cells and may serve as vehicles for the transfer of protein and RNA among cells.
SKOV3 exosomes were labelled with carboxyfluoresceine diacetate succinimidyl-ester and collected by ultracentrifugation. Uptake of these vesicles, under different conditions, by the same cells from where they originated was monitored by immunofluorescence microscopy and flow cytometry analysis. Lectin analysis was performed to investigate the glycosylation properties of proteins from exosomes and cellular extracts.
In this work, the ovarian carcinoma SKOV3 cell line has been shown to internalize exosomes from the same cells via several endocytic pathways that were strongly inhibited at 4°C, indicating their energy dependence. Partial colocalization with the endosome marker EEA1 and inhibition by chlorpromazine suggested the involvement of clathrin-dependent endocytosis. Furthermore, uptake inhibition in the presence of 5-ethyl-N-isopropyl amiloride, cytochalasin D and methyl-beta-cyclodextrin suggested the involvement of additional endocytic pathways. The uptake required proteins from the exosomes and from the cells since it was inhibited after proteinase K treatments. The exosomes were found to be enriched in specific mannose- and sialic acid-containing glycoproteins. Sialic acid removal caused a small but non-significant increase in uptake. Furthermore, the monosaccharides D-galactose, α-L-fucose, α-D-mannose, D-N-acetylglucosamine and the disaccharide β-lactose reduced exosomes uptake to a comparable extent as the control D-glucose.
In conclusion, exosomes are internalized by ovarian tumor cells via various endocytic pathways and proteins from exosomes and cells are required for uptake. On the other hand, exosomes are enriched in specific glycoproteins that may constitute exosome markers. This work contributes to the knowledge about the properties and dynamics of exosomes in cancer.
Exosomes are small membrane vesicles between 40-100 nm in diameter that are secreted by various cell types, including tumor cells, neurons, B- and T- lymphocytes, intestinal epithelial cells [1–3] and in physiological fluids [3, 4].
Exosome biogenesis involves the inward budding of endosomes into multivesicular bodies to form intraluminal vesicles that are then released to the extracellular space. During this process transmembrane proteins are incorporated into the invaginating membrane maintaining the same topological orientation as the plasma membrane, while cytosolic components are engulfed.
The molecular basis of protein sorting during exosomes formation appears to involve a ubiquitin-dependent mechanism and the endosomal sorting complexes required for transport (ESCRT) [5, 6]. However, some proteins present in the exosomes are not ubiquitinated suggesting that other mechanisms such as oligomerization or partitioning of protein into lipid raft domains may be involved [6–9].
Exosomes are released by multivesicular bodies fusion with the plasma membrane and the mechanism appears to involve Rab27A and Rab27B . Recent studies have suggested their participation in different physiological and/or pathological processes, such as, tumor progression, stimulation of the immune system, coagulation and inflammation and intercellular transfer of infectious agents, such as proteins and RNA [4, 6, 8].
Many of the functions described for exosomes depend on their ability to specifically interact with a target cell and several types of interaction have already been proposed based on indirect evidence and in vitro studies. Exosomes can associate with the plasma membrane through ligand-receptor interactions  or lipids, such as phosphatidylserine . The process of internalization can occur through direct fusion of the exosomes with the plasma membrane, leading to the release of the exosomal content into the cell cytoplasm. Alternatively, exosomes can enter the cells by receptor-mediated endocytosis and later fuse with the limiting membrane of the endosome releasing the exosomal content to be recycled to the cell surface or to be degraded in the lysosome [11, 13]. Exosome uptake was shown to occur via clathrin-mediated endocytosis in dendritic cells , as well as phagocytosis in monocytes and macrophages .
Exosomes have a unique protein and lipid composition that varies depending on the cells from which they originate, nevertheless, as a consequence of their endosomal origin nearly all exosomes contain proteins involved in membrane transport and fusion (RabGTPases, annexins, flotilin), in multivesicular bodies biogenesis (TSG101, Alix), heat shock proteins (Hsc70, Hsc90), integrins and tetraspanins (CD9, CD63, CD81, CD82) [16, 17]. In addition, they are enriched in raft-lipids such as cholesterol, sphingolipids and ceramide. In exosomes, an enrichment of certain glycosylated motifs has also been observed .
Glycosylation is a post-translational modification that plays an important role in several properties of proteins including stability, folding, intracellular trafficking and recognition. Lectins and their interactions with carbohydrates have been found to play a role in exosome uptake by dendritic cells  and macrophages .
In the present work, the SKOV3 ovarian carcinoma cell line has been shown to internalize exosomes derived from the same cells via various endocytic pathways. Proteins from exosomes and from cells were required for the uptake. On the other hand, exosomes were highly enriched in specific glycosylated sialic acid- and mannose-containing glycoproteins, and sialic acid removal caused a small though non-significant increase in uptake.
Human ovarian cancer SKOV3, embryonic kidney HEK293 and neuroglioma H4 cell lines were grown in Dulbecco's Modified Eagle Medium (DMEM) (Sigma) at 37°C, 5% CO2 supplemented with 10% fetal calf serum (Gibco), 1% penicillin/streptomycin solution (Gibco).
Isolation of secreted membrane vesicles
Confluent SKOV3, HEK293 and H4 cells were cultivated for 24 h in serum-free medium. The supernatant was collected and centrifuged, at 500, 10,000 and 100,000 × g 10, 20 and 120 min, respectively, at 4°C. The pellet of the last centrifugation consisted of secreted membrane vesicles. Sucrose-density-fractionation was performed as described previously .
Glycoprotein detection using lectins and immunoblot
Cellular extracts were obtained by solubilization of centrifuged cells in Triton X-100 buffer (50 mM Tris-HCl pH 7.5, 5 mM EDTA, 1% Triton X-100, 0.02% protease inhibitors cocktail, Complete, Roche), for 30 min. Total protein concentration was determined by the bicinchoninic acid (BCA) method.
Glycoproteins from total cellular extracts and secreted membrane vesicles were stained after transfer to polyvinylidene difluoride (PVDF) membrane with lectins. Concanavalin A (Con A) (Sigma), biotinylated Sambucus nigra (SNA) and Maackia amurensis lectin (MAL) (Galab Technologies) were used. Glycoproteins were fixed on the PVDF membrane with 25% (v/v) 2-propanol and 10% (v/v) acetic acid for 5 min. The membranes were blocked for 1 h with TBS, 0.1% Tween-20 (TTBS) for Con A or with TTBS containing 2% BSA for SNA and MAL. For Con A detection the membrane was incubated overnight with 25 μg/ml Con A in TTBS containing 1 mM CaCl2 and 1 mM MgCl2 (TTBSS) followed by 1 h incubation with 0.5 μg/ml horseradish peroxidase type I (Sigma) in TTBSS. For SNA and MAL detection, membranes were incubated overnight in TTBS with 0.5 or 5 μg/ml SNA or MAL lectin, respectively. Membranes were further incubated for 1 h with 0.02 μg/ml streptavidin-peroxidase (Sigma). Detection was performed with the Immobilon Western chemiluminescent HRP substrate (ECL) (Millipore).
Immunoblot was performed as previously described . The following antibodies were used: mouse anti-CD9 (1:5000) and mouse anti-L1 (L1-11A) (1:3).
Hydrolysis of α2,3- and α2,6-linked NeuAc from total protein cellular extracts and exosomes was carried out overnight at 37°C by the addition of 15 mU neuraminidase from Vibrio cholerae or from Arthrobacter urefaciens (Roche) in 50 mM sodium acetate pH 5.5 containing 4 mM CaCl2, and 50 mM sodium acetate pH 5.0, respectively. For specific hydrolysis of α2,3-linked NeuAc, 9 U neuraminidase from Streptococcus pneumoniae (Prozyme, Glyko) in 50 mM sodium phosphate pH 6.0 were used, for 1 hour at 37°C.
Uptake of SKOV3 exosomes by SKOV3 cells
SKOV3 exosomes were labeled with carboxyfluoresceine diacetate succinimidyl-ester (CFSE) (Invitrogen) as previously described . Briefly, exosomes (20 μg) collected after a 100,000 × g ultracentrifugation were incubated with 7.5 μM CFSE for 30 min at 37°C in a final volume of 200 μl PBS containing 0.5% BSA. Labeled exosomes (Exos-CFSE) were 65-fold diluted with DMEM supplemented with 10% vesicles-free fetal calf serum and pelleted by ultracentrifugation for 16 h at 10,0000 × g, 12°C. Exos-CFSE were resuspended in DMEM and incubated with SKOV3 cells at 37 or 4°C.
When indicated Exos-CFSE or cells were treated for 30 min with 100 μg/ml proteinase K, or for 2 h with 15 mU neuraminidase from V. cholerae or from A. urefaciens (Roche), before uptake. SKOV3 cells were also incubated, 30 min prior to and during uptake, with the inhibitors 10 μg/ml chlorpromazine, 5 μg/ml cytochalasin D, 50 μM 5-ethyl-N-isopropyl amiloride (EIPA) or 2% methyl-beta-cyclodextrin, or with 150 mM of the monosaccharides D-glucose, D-galactose, α-L-fucose, α-D-mannose, D-N-acetylglucosamine, and the disaccharide β-lactose (Sigma).
Uptake assays were always performed in the presence of the compounds and analyzed after 2 or 4 h by immunofluorescence microscopy or flow cytometry.
Immunofluorescence microscopy was done as previously described . Primary antibodies were: mouse IgG anti-alpha-tubulin DM1A (1:2000) (Sigma), mouse IgG anti-EEA1 (1:100) (BD Biosciences), mouse IgG anti-LAMP1 H4A3 (1:100) (BD Biosciences) and mouse IgG anti-caveolin-1 (1:50) (Santa Cruz). Secondary antibody was donkey anti-mouse IgG AlexaFluor 594 (1:500) (Molecular Probes).
Images were acquired on a Leica DMRB microscope using a DFC340FX camera coupled to the microscope, and Leica application suite V3.3.0 software. For colocalization, images were acquired on a confocal SP5 microscope. Each picture was acquired with laser intensities and amplifier gains adjusted to avoid pixel saturation. Each fluorophore used was excited independently and sequential detection was performed. Each picture consisted of a z-series of 20 images of 1024-1024 pixel resolution with a pinhole of 1.0 airy unit. Colocalization analysis was performed using the open source Image J version 1.38 http://rsb.info.nih.gov/ij/.
SKOV3 cells incubated with Exos-CFSE for 4 h at 37 or 4°C were washed with PBS, detached using trypsin and resuspended in PBS with 2% fetal calf serum (Gibco). Flow cytometry analysis was performed on a Cyflow ML cytometer (Partec) using Flowmax software 2.56 (Partec). Gate was set on living cells based on forward/side scatter properties and a minimum of 103 events within the gated live population were collected per sample. Exos-CFSE uptake by SKOV3 cells was measured by the shift in peak fluorescence intensity of CFSE, calculated by the geometric mean of the population. SKOV3 cells with no Exos-CFSE uptake (unlabelled) were used as controls for cell autofluorescence. Results were expressed as means ± S.D. and comparison between two means was performed by Student t test. A P value lower than 0.05 was considered significant.
Uptake of SKOV3 exosomes by SKOV3 cells
Since it has been shown that SKOV3 exosomes can be internalized by NK cells  here we have investigated if they are internalized by the cell line from where they originated. With that purpose exosomes produced in the absence of fetal bovine serum and collected at 100,000 × g were labeled with CFSE (Exos-CFSE) and incubated with SKOV3 cells. CFSE is a membrane permeable non-fluorescent compound that becomes fluorescent after cleavage of its acetate groups by intracellular esterases . A punctuated green fluorescent pattern corresponding to Exos-CFSE interaction/internalization was observed after 30 min and it increased up to 4 hours of incubation (Figure 1A). To obtain a higher sensitivity exosomes were also biotinylated and detected with streptavidin Alexa-488, and the interaction was observed already 0.5 min after incubation (data not shown). Colocalization studies by immunofluorescence confocal microscopy of Exos-CFSE and alpha-tubulin, a microtubule marker, showed that Exos-CFSE were localized in the same z-stacks as microtubules, thus, confirming their internalization (Figure 1B). Supporting this conclusion was the observation that the exosomes were not removed by acid wash of cells pre-exposed to Exos-CFSE (data not shown).
Several endocytic mechanisms have been described to mediate the entry of material into the cells . Here, we observed that a decrease in temperature from 37 to 4°C caused a reduction of 80 ± 8% (n = 6) in the number of labeled cells as well as a decrease of 77 ± 9% (n = 6) in the uptake for the positively labeled cells, based on the shift in fluorescence intensity corresponding to the geometric mean of the population peaks (Figure 2A). These results indicated that exosomes uptake was mediated by endocytosis in an energy-dependent process. Exos-CFSE were also found to partially colocalize with the endosomal marker EEA1 (Figure 2B), thus showing the participation of clathrin-mediated endocytosis in exosome uptake. This conclusion was further supported by uptake inhibition (19 ± 18%, n = 4) (Figure 2C) with 10 μg/ml chlorpromazine, which blocks clathrin-mediated endocytosis . Colocalization with the lysosomal marker LAMP1 (Figure 2B) indicated that at least a part of the exosomes were targeted to the lysosome.
In addition other inhibitors have been tested. First, cells incubated with 5 μg/ml cytochalasin D, which is known to inhibit actin polymerization and consequently inhibit phagocytosis  as well as other endocytic pathways  showed an uptake reduction of 32 ± 7% (n = 4) (Figure 2C). EIPA at 50 μM, which is known to block macropinocytosis , caused an uptake reduction of 36 ± 13% (n = 5) (Figure 2C), thus suggesting that exosomes were internalized via macropinocytosis. Methyl-beta-cyclodextrin, that is used to deplete cholesterol from cellular membranes , decreased Exos-CFSE uptake (44 ± 8%, n = 5) (Figure 2C). However, there was no colocalization with caveolin-1 (Figure 2B), which is a marker of caveolae that are enriched in cholesterol rich domains. These results indicated that exosome uptake could occur via a cholesterol associated pathway independent of caveolae or that methyl-beta-cyclodextrin affected exosomes membrane integrity, thus decreasing uptake efficiency.
Exos-CFSE did not colocalize with the Golgi marker GM130, the trans-Golgi network marker TGN46 or the endoplasmic reticulum marker calnexin (data not shown).
Proteins are required for exosomes uptake
The recognition between exosomes and the target cell has been reported to involve proteins present at the cell surface of both exosomes and target cells [11, 14]. Here, Exos-CFSE or SKOV3 cells were digested with proteinase K, a broad specificity protease, and uptake efficiency was analyzed by flow cytometry analysis. Uptake levels of digested Exos-CFSE were found to be lower (45 ± 12%, n = 6) than Exos-CFSE without treatment (Figure 3A). As control, fluorescence of Exos-CFSE was not affected by proteinase K treatment (data not shown). Furthermore, a decrease of 32 ± 8% (n = 6) in uptake was observed in SKOV3 cells treated with proteinase K (Figure 3B). Therefore, proteins present in exosomes and also in SKOV3 cells are required, at least in part, for internalization by target cells.
Enrichment of specific glycoproteins in exosomes and relevance in uptake
Glycan-lectin interactions have been suggested to play a role in the uptake of exosomes by target cells [19, 20], therefore, we have investigated if glycans would play a role in exosome uptake by SKOV3 cells.
First, glycoproteins of cellular extracts and secreted vesicles from SKOV3 cells were detected with the lectins concanavalin A (Con A; binds α-mannosyl containing-branched glycans predominantly of the high-mannose followed by hybrid- and biantennary complex type structures to a lower extent) , Sambucus nigra lectin (SNA; recognizes NeuAcα2,6Gal/GalNAc) and Maackia amurensis lectin (MAL; binds NeuAcα2,3Galβ1,4GlcNAc/Glc) . The profile from exosomes was distinct from that of cellular extracts with the three lectins (Figure 4A). Detection with SNA and MAL was almost totally abolished after digestion with V. Cholerae and A. urefaciens neuraminidases (cleave terminal α2,3- and α2,6-linked NeuAc), whereas only MAL binding was abolished after S. pneumoniae (cleaves only α2,3-linked NeuAc) digestion (Figure 4B), thus confirming that SNA and MAL binding to secreted vesicles glycoproteins was specific. The sialic acid was not present in sialylated Lewis epitopes, since there was no detection with anti-sialyl-Lewisa or anti- sialyl-Lewisx antibodies (data not shown).
SKOV3 secreted vesicles are constituted by exosomes and apoptotic vesicles, which can be fractionated by using a sucrose gradient, as previously described [21, 22]. CD9 is a tetraspanin protein that has been used as exosome marker [32, 33]. After sucrose gradient separation of the secreted vesicles all the SNA and MAL binding was found in the exosome-containing fractions (fractions 2-5) and not in the apoptotic blebs (fractions 8-11) (Figure 4C).
Specific patterns of protein glycosylation were also found for exosomes from two other human cell lines, embryonic kidney HEK293 and neuroglioma H4 cells (Figure 5).
To investigate a possible role for glycosylation in exosome uptake Exos-CFSE were desialylated with V. cholerae and A. urefaciaens sialidases and exosomes uptake was monitored by immunofluorescence microscopy and flow cytometry analysis of cell fluorescence intensity. Uptake efficiency of exosomes after neuraminidase treatment was slightly increased (16 ± 14%, n = 6) when compared with exosomes incubated with neuraminidase buffer (Figure 6A), however, the observed increase was not statistically significant using the Student t test (P = 0.0764). In addition, increases in the uptake of exosomes incubated with neuraminidase (38 ± 13%, n = 6) or neuraminidase buffer (23 ± 14%, n = 6) were detected when compared with Exos-CFSE without treatment (Figure 6A).
The uptake assay was also performed in the presence of 150 mM of the monosaccharides D-glucose (control), D-galactose, α-L-fucose, α-D-mannose and D-N-acetylglucosamine, and the disaccharide β-lactose. Decreases of 23 ± 7%, 24 ± 14%, 25 ± 16%, 27 ± 8%, 19 ± 15% and 20 ± 8% (n = 6), respectively, in the uptake of Exos-CFSE in comparison with control without sugar were observed. The incubation with α-D-mannose led to a higher decrease in uptake relatively to the control sugar D-glucose, however the difference was not statistically significant (Figure 6B).
Exosomes are small membrane vesicles that are secreted by several cell types, including tumors and they have been found in biological fluids. They contain several membrane and cytoplasmic proteins and, in cancer, they play a role in cell migration and metastases. They may also transfer proteins associated with deregulated signalling pathways in cancer [34, 35], therefore, contributing to the propagation of transformed phenotype. Furthermore, the exosomes may transfer mRNA and miRNA .
In the present work, we have found that the SKOV3 ovarian carcinoma cell line internalizes exosomes derived from the same cells in an energy-dependent process, via various endocytic pathways: colocalization studies with organelle markers and incubation with inhibitors have shown that the endocytosis pathway dependent on clathrin, macropinocytosis and a cholesterol associated pathway independent of caveolae were associated with the uptake. Evidence from the literature showed that in dendritic cells exosome uptake was also inhibited at 4°C and with cytochalasin D, and was further trafficked to the late endosomes/lysosomes . In phagocytic cells, more specifically macrophages, internalization was also dependent on the actin cytoskeleton but not on pathways involving caveolae, macropinocytosis or clathrin-coated vesicles . In the PC12 cell line exosomes uptake was also found to occur via the endocytic pathway . After internalization, exosomes could fuse with the endosomal membrane and deliver their content to the cytoplasm of the target cell. For SKOV3 cells such process could take place over a long period of time since internalized exosomes were detected in the cells for at least 20 h (data not shown).
The initial recognition events that precede uptake may involve several molecules, proteins  and lipids  have already been indicated as involved in this process. In this work, the impairment observed for vesicles or cells treated with proteinase K indicated that proteins from the extracellular surface from both target cells and exosomes are required for internalization. Further studies to identify which proteins play an important role in the recognition are required.
Here we also found that exosomes from SKOV3 cells are particularly enriched in specific glycoproteins with high-mannose or NeuAcα2,3/6-containing structures. In this context, other authors, using lectin arrays, have also observed the enrichment in T-cells secreted microvesicles of high-mannose and sialic acid-containing structures in comparison with cell membranes . Furthermore, an enrichment of more extensively glycosylated forms of PrPc has been found in the exosomes in comparison with cell lysates .
Removal of NeuAc from the exosomes with neuraminidase led to an increase in the uptake, but non-significant. The removal of NeuAc decreased the negative charge at the exosome surface exposing galactose or N-acetylgalactosamine residues. This could lead to physico-chemical alterations of the membrane or create new ligands for carbohydrate binding proteins at the surface of the cells that would mediate the binding.
The monosaccharides D-galactose, α-L-fucose, α-D-mannose, D-N-acetylglucosamine and the disaccharide β-lactose reduced exosomes uptake to a comparable extent as the control D-glucose probably due to increased osmotic pressure that is known to reduce endocytosis . Therefore, these sugars do not play a major role in exosome interaction and uptake in SKOV3 cells. This result is different from that found in dendritic cells where exosome uptake was specifically inhibited by mannose and N-acetylglucosamine, the interaction being at least in part mediated by a C-type lectin , or in macrophages where lactose diminished exosome uptake probably through its action on galectin-5 that mediated the process .
Here, certain glycoproteins were specifically detected in exosomes and may constitute markers. It will be interesting to investigate if those glycoproteins are selectively sorted to the exosomes or if only certain glycoforms from the same protein are sorted into the exosomes. It can be admitted that glycans by themselves may be important for glycoprotein sorting into exosomes. Since protein oligomerization is known to promote sorting into exosomes independently of the ESCRT machinery and ubiquitination , the glycans could mediate oligomerization via interaction with lectins as previously described for the transferrin receptor in reticulocytes . Moreover, glycans may interact with galectins at the cell surface, which may lead to their enrichment in membrane lipid domains as previously described . Considering that lipid microdomains play a role on exosomes biogenesis , glycans could in that case also have a role on sorting to exosomes. Further studies are required to clarify this matter.
Exosomes contain cell surface cancer antigens, which confers them the potential for therapeutic approaches in cancer vaccination. Our observation that they are particularly enriched in glycan epitopes urges the need to further characterize the corresponding structures since one of the major changes that occur in cancer is in cell surface glycosylation, which has been largely used as biomarker. The knowledge of exosomes glycosylation with the possibility for its modulation will open new perspectives in cancer vaccination.
Exosomes secreted by the ovarian cancer SKOV3 cell line are internalized by the same cells, and internalization is energy-dependent and it occurs via various endocytic pathways. Moreover, the interaction requires proteins from the cells and the exosomes. On the other hand, the exosomes were found to be enriched in specific mannose- and sialic acid-containing glycoproteins that could constitute exosome markers. Furthermore, sialic acid removal caused a small though non-significant increase in uptake.
- Con A:
Sambucus nigra lectin
Maackia amurensis lectin
carboxyfluoresceine diacetate succinimidyl-ester
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The pre-publication history for this paper can be accessed here:http://www.biomedcentral.com/1471-2407/11/108/prepub
We thank the Cell Imaging Service (Instituto Gulbenkian de Ciência, Portugal) for the use of the confocal microscope; Dr. Paula Alves and Dr. Catarina Brito (Instituto de Biologia Experimental e Tecnológica, Portugal) for the use of the flow cytometer; Dr. Rui Gardner (Instituto Gulbenkian de Ciência) for helpful discussion; Dr. Tiago Outeiro, Instituto de Medicina Molecular, Lisbon, for the gift of the H4 cell line.
This work was funded by projects Signalling and Traffic, No. LSHG-CT-2004-503228, CellPROM, No. 500039-2, European Commission, and PIC/IC/82765/2007, PTDC/SAU-NEU/100724/2008, Fundação para a Ciência e a Tecnologia, Portugal. CE had a Ph.D. fellowship from Fundação para a Ciência e a Tecnologia.
The authors declare that they have no competing interests.
CE contributed to study design, data interpretation, carried out the experiments and prepared the manuscript. SK contributed to experimental work and data interpretation. PA contributed to study design, data interpretation and manuscript revision. JC coordinated the study design, data interpretation and manuscript revision. All authors have read and approved the final manuscript.
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Escrevente, C., Keller, S., Altevogt, P. et al. Interaction and uptake of exosomes by ovarian cancer cells. BMC Cancer 11, 108 (2011). https://doi.org/10.1186/1471-2407-11-108