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Mesenchymal Stromal Cells Epithelial Transition Induced by Renal Tubular Cells-Derived Extracellular Vesicles

Mesenchymal Stromal Cells Epithelial Transition Induced by Renal Tubular Cells-Derived Extracellular Vesicles

  • Giulia Chiabotto, 
  • Stefania Bruno, 
  • Federica Collino, 
  • Giovanni Camussi
PLOS
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Abstract

Mesenchymal-epithelial interactions play an important role in renal tubular morphogenesis and in maintaining the structure of the kidney. The aim of this study was to investigate whether extracellular vesicles (EVs) produced by human renal proximal tubular epithelial cells (RPTECs) may induce mesenchymal-epithelial transition of bone marrow-derived mesenchymal stromal cells (MSCs). To test this hypothesis, we characterized the phenotype and the RNA content of EVs and we evaluated the in vitro uptake and activity of EVs on MSCs. MicroRNA (miRNA) analysis suggested the possible implication of the miR-200 family carried by EVs in the epithelial commitment of MSCs. Bone marrow-derived MSCs were incubated with EVs, or RPTEC-derived total conditioned medium, or conditioned medium depleted of EVs. As a positive control, MSCs were co-cultured in a transwell system with RPTECs. Epithelial commitment of MSCs was assessed by real time PCR and by immunofluorescence analysis of cellular expression of specific mesenchymal and epithelial markers. After one week of incubation with EVs and total conditioned medium, we observed mesenchymal-epithelial transition in MSCs. Stimulation with conditioned medium depleted of EVs did not induce any change in mesenchymal and epithelial gene expression. Since EVs were found to contain the miR-200 family, we transfected MSCs using synthetic miR-200 mimics. After one week of transfection, mesenchymal-epithelial transition was induced in MSCs. In conclusion, miR-200 carrying EVs released from RPTECs induce the epithelial commitment of MSCs that may contribute to their regenerative potential. Based on experiments of MSC transfection with miR-200 mimics, we suggested that the miR-200 family may be involved in mesenchymal-epithelial transition of MSCs.

Introduction

Mutual interactions between epithelial cells and mesenchymal cells coordinate kidney development, play a pivotal role in maintaining organ integrity in the adult, and contribute to renal regeneration after injury. Bone marrow-derived mesenchymal stromal cells (MSCs) have multipotent characteristics, since they can differentiate into adipocytes, osteocytes and chondrocytes. Moreover, the epithelial commitment of bone marrow-derived MSCs induced by renal tubular epithelial cells has been demonstrated in co-culture conditions [1]. Recently, conditioned medium derived from renal tubular epithelial cells has also proved to induce an epithelial commitment of adipose-derived adult MSCs [2] and of bone marrow-derived MSCs [3,4].

The epithelial reprogramming of MSCs consists in the acquisition of morphological, antigenic and functional properties of polarized epithelial cells. Mesenchymal-epithelial transition (MET) has been defined as an activation of epithelial genes, including those encoding for cytokeratins, desmosomes, adherens and tight junctions, and an inactivation of mesenchymal genes, such as vimentin and collagen [5]. MET is a phenomenon observed during nephrogenesis, when the metanephric mesenchyme develops into nephrons [6]. During embryogenesis, both MET and epithelial-mesenchymal transition (EMT)—the reversed program of MET—are essential for organ development. While there are plenty of studies analyzing EMT related to fibrosis in chronic inflammation and metastasis of tumor [713], relatively little is known about MET associated with kidney formation. This process seems to be regulated by genes such as paired box 2 (PAX2), bone morphogenetic protein 7 (BMP7), and Wilms tumor 1 (WT1) [1416].

Besides physical interactions, such as direct cell-to-cell contact, nanotubes and cytonemes, and the release of soluble factors, the extracellular vesicles (EVs) have recently emerged as an important mechanism of communication between cells. The term EVs includes exosomes, originating from the membrane of the endosomal compartment, and microvesicles, derived from plasma membrane budding. Both of them are small membrane fragments that can shuttle cytosolic proteins, receptors, bioactive lipids and nucleic acids to target cells, acting as a potent paracrine mechanism that can re-direct cell fate [17]. Ratajczak et al.[18] first described that EVs derived from embryonic stem cells may reprogram hematopoietic progenitors by a mRNA-dependent mechanism. Quesenberry and Aliotta suggested that a continuous genetic modulation of cells through transfer of EVs may be involved in the continuum change in bone marrow stem cell phenotype. EV-mediated transfer of proteins and genetic information from injured cells to bone marrow-derived stem cells may reprogram their phenotype to acquire features of the injured tissue [19,20].

EVs carry proteins, lipids, and nucleic acids, including microRNAs (miRNAs) [2123] short non-coding RNAs that regulate post-transcriptional expression of several genes, either by triggering mRNA cleavage or by repressing translation [24,25].

The aim of the present study was to evaluate whether renal tubular epithelial cell (RPTEC)-derived EVs are involved in the epithelial differentiation of bone marrow-derived MSCs and the role of miRNAs carried by EVs.

Materials and Methods

Cell culture

Human bone marrow-derived MSCs were obtained from Lonza (Basel, Switzerland), cultured and characterized as previously described [26,27]. Briefly, MSCs were cultured in the presence of Mesenchymal Stem Cells Basal Medium (MSCBM, Lonza) and maintained in an incubator with a humidified atmosphere of 5% CO2 at 37°C. MSCs were seeded at a density of 10,000 cells/cm2 and used within the seventh passage. The adipogenic, osteogenic and chondrogenic differentiation ability of MSCs was determined as previously described [26,27].

Human RPTECs were obtained from Lonza and cultured in Renal Epithelial Cell Basal Medium (REBM, Lonza) supplemented with Renal Epithelial Cell Growth Medium Bullet Kit (REGM, Lonza), according to the manufacturer’s instructions.

Immunofluorescence analyses

Indirect immunofluorescence was performed on cells cultured on chamber slides (Nalgen Nunc International, Rochester, NY, USA). The cells were fixed in 2,5% paraformaldehyde and permeabilized with Hepes-Triton X100 buffer (Sigma-Aldrich, St. Louis, MO). The following antibodies were used: mouse monoclonal anti-vimentin (Sigma-Aldrich), mouse monoclonal anti-pan-cytokeratin (Bio-Rad, Hercules, CA), rabbit polyclonal anti-cytokeratin 18 and goat polyclonal anti-aminopeptidase A (Santa Cruz Biotechnology, Dallas, TX). As a control, primary antibodies were omitted and substituted with nonimmune mouse IgG. Alexa Fluor 488 anti-mouse (Invitrogen, Carlsbad, CA) was used as secondary antibody. For nuclear staining, Hoechst 33258 dye (Sigma-Aldrich) was added to fixed cells. A Zeiss LSM 5 Pascal Model Confocal Microscope (Carl Zeiss International, Germany) was used to perform confocal microscopy analysis.

MSCs expressed high levels of vimentin (S1A Fig), while cytokeratins expression was not detected (S1B Fig). RPTECs expressed low levels of vimentin (S2A Fig) and high levels of cytokeratins (S2B Fig).

Cytofluorimetric analyses

Cells were counted at each passage and their immunophenotype was analyzed by cytofluorimetric analysis, using FACS Calibur (BD Biosciences, San Jose, CA). The following antibodies, all fluorescein isothiocyanate (FITC) or phycoerythrin (PE) conjugated were used: anti-CD105, -CD146 (Miltenyi Biotech, Bergisch Gladbach, Germany); -CD29, -CD44, -CD45, -alpha5 integrin (CD49e), -alpha6 integrin (CD49f), -CD73, -CD90, -VEGFR2 (Becton Dickinson Biosciences Pharmingen, San Jose, CA); -EpCAM, -HLA-I (BioLegend, San Diego, CA). Mouse IgG isotypic controls were from Miltenyi.

MSCs showed the expression of typical MSC surface marker molecules: CD29 (integrin beta-1), CD44, CD73 (ecto-5’-nucleotidase), CD90 (Thy-1 cell surface antigen), CD105 (endoglin) and CD146 (melanoma cell adhesion molecule, MCAM), while epithelial marker EpCAM was not detected (S1C Fig).

RPTECs showed the expression of CD24, CD29, CD44, alpha-5 integrin (CD49e), alpha-6 integrin (CD49f), CD73, CD146, EpCAM, and HLA-class I surface molecules while hematopoietic marker CD45, endothelial marker VEGFR2, and mesenchymal stromal cell marker CD105 were not detected (S2C Fig).

Extracellular vesicles isolation and conditioned medium preparation

EVs were obtained from supernatant of ≥80% confluent RPTECs cultured overnight in RPMI (without phenol red, Invitrogen) supplemented with 2% FBS deprived of EVs after 15 hours of centrifugation at 100,000 g (Optima L-90K ultracentrifuge, Beckman Coulter, Indianapolis, IN). Cell supernatant was collected, centrifuged at 2,000 g for 20 minutes to remove debris, and processed to obtain: (1) extracellular vesicles (EVs), (2) total conditioned medium with EVs (TOT-CM) and (3) conditioned medium after EVs deprivation (CM) after ultracentrifugation at 100,000 g for 15 hours.

EVs were isolated from cell-free supernatant by differential ultracentrifugation as previously described by Théry and colleagues [28]. The pellet collected after ultracentrifugation at 100,000 g was resuspended in RPMI containing 10% dimethyl sulfoxide (DMSO, Sigma-Aldrich) and stored at -80°C.

Particles size and concentration were measured by NanoSight LM10 instrument (NanoSight Ltd, Amesbury, UK) equipped with the nanoparticle tracking analyses (NTA) 2.0 analytic software [29,30].

TOT-CM and CM were concentrated ~20-fold by centrifugation at 2,700 g for 40 minutes at 4°C, using ultrafiltration units with a 3 kDa molecular weight cut-off (Amicon Ultra -15, centrifugal filter devices, Millipore, Billerica, MA). To preserve EVs integrity, TOT-CM was supplemented with 10% DMSO and stored at -80°C, while CM was stored directly at -20°C.

EV characterization

Cytofluorimetric analysis was performed as previously described [30,31]. Briefly, EVs were incubated for 15 minutes at 4°C with the following FITC- or PE-conjugated antibodies: anti-CD24, -CD29, -CD44, -alpha5 integrin (CD49e), -alpha6 integrin (CD49f), -CD63, -CD73, -CD81, -CD107, (Becton Dickinson), -CD146, -EpCAM, -HLA1 (BioLegend, San Diego, CA). FITC or PE mouse nonimmune isotypic IgG (Miltenyi) were used as control. For each EV preparation, 5,000 particles were acquired using Guava easyCyte™ Flow Cytometer (Millipore) and analysed with the InCyte™ software.

Incorporation of EVs in MSCs

To study EVs incorporation by MSCs, we incubated these cells with 30,000 labelled-EVs/cell for 6-15-24 hours at 37°C. The EVs were previously stained with a red-fluorescent dye which binds to lipid membranes (Vybrant™ DiI cell-labeling solution, Invitrogen), in accordance with the manufacturer’s instructions. Hoechst 33258 (Sigma-Aldrich) staining was used to visualize cellular nuclei. EVs uptake was evaluated by confocal microscopy.

Stimulation experiments using RPTEC-derived EVs, or TOT-CM or CM and co-culture experiments

To test the role of RPTEC-derived paracrine factors in MSC differentiation, MSCs were seeded in MSCBM, at a density of 50,000 cells/well in 6-well plates (Becton Dickinson) and stimulated with 150,000 EVs/cell, 30% CM, or 30% TOT-CM for 7–14 days before RNA extraction. When using TOT-CM to stimulate MSCs, we maintained the same ratio EV:cells that we used to stimulate MSCs with EVs. For co-culture experiments, a transwell system with a 1 μm pore size permeable membrane (Becton Dickinson) was used to separate RPTECs physically from bone marrow MSCs in 6-well plates (Becton Dickinson). RPTECs were seeded into the upper insert of the transwell system in DMEM with 5% FBS, at a density of 100,000 cells/well. MSCs were seeded into the lower chamber of this co-culture system, at a density of 50,000 cells/well. MSCs cultured alone in MSCBM were used as control. Cells were maintained in co-culture conditions for 7 days before RNA extraction. Six different experiments with similar results were done.

Trans-epithelial electric resistance

Trans-epithelial electrical resistance (TEER) was used as an indicator of epithelial differentiation and integrity (30). Control MSCs, or MSCs cultured in the presence of EVs or TOT-CM, or MSCs co-cultured with RPTECs were plated on polycarbonate membrane transwell (Falcon Corning Corp., Cambridge, MA) and allowed to reach confluency. An epithelial volt-ohm meter (EVOM, World Precision Instruments, Inc., Sarasota, FL) was used to determine the TEER. Measurement of cell-free membrane inserts were performed and subtracted from all subsequent measurement and expressed as ohm/cm2. All values were normalized for the area of the membrane. All experiments were done in triplicate.

Albumin uptake

Cellular uptake of albumin was analyzed in confluent MSC monolayers using fluorescein isothiocyanate (FITC)-labeled albumin (Sigma-Aldrich), as previously described [32]. Briefly, after 14 days of co-culture with RPTECs or stimulation with EVs or TOT-CM, cell medium was refreshed and MSCs were incubated with 50 μg/ml of FITC-labeled BSA (Sigma-Aldrich) for two hours at 37°C. Fluorescence emission was measured by cytofluorimetric analysis.

Western Blot Analysis

For protein analysis, EVs and cells were lysed at 4°C for 30 minutes in RIPA buffer (20 nM Tris-HCl, 150 nM NaCl, 1% deoxycholate, 0.1% SDS, 1% Triton X-100, pH 7.8) supplemented with PMSF, protease and phosphatase inhibitors cocktail (Sigma-Aldrich). EV samples were quantified using a proteic Bradford assay. Since the EVs protein concentration was lower than 2 mg/ml, a mixture of methanol-chloroform-water was used for the quantitative precipitation of proteins, as previously described [33,34]. Aliquots of the cell lysates containing 30 μg proteins were run on 10% acrylamide gel SDS-PAGE under reducing conditions. Proteins were transferred onto a PVDF membrane using the 7 minutes transfer program of the iBlot™ Dry Blotting System (Life Technology, Carlsbad, CA). The blots were blocked with 5% non fat milk in PBS supplemented with 0.1% Tween-20 (PBS-T). The following primary antibodies were used at 1∶200 dilution: anti-human aminopeptidase A and anti-human pan-cytokeratin (Santa Cruz Biotechnology). After incubation for 15 hours at 4°C with primary antibodies, membranes were washed with PBS-T and then incubated with for one hour at room temperature with peroxydase conjugated secondary antibodies (Santa Cruz Biotechnology). Finally, membranes were washed with PBS-T, developed with ECL detection reagents (GE healthcare, Amersham, Buckinghamshire, UK) and detected by Chemidoc XRS system (Bio-Rad).

RNA extraction and quantitative Real Time Reverse Transcriptase Polymerase Chain Reaction

Total RNA was isolated from both EVs and cells (used in co-culture and stimulation experiments) using miRNeasy mini kit (Qiagen, Valencia, CA), according to manufacturer’s instructions, and quantified spectrophotometrically (Nanodrop ND-1000, Wilmington DE). The quality of EVs-derived RNA was evaluated by capillary electrophoresis on an Agilent 2100 Bioanalyzer (Agilent Technologies, Inc, Santa Clara, CA) using the eukaryotic total RNA 6000 Pico Kit. The presence of small RNAs was verified in both EV and cell samples using the Small RNA Kit (Agilent Tech).

The mRNA expression in MSCs co-cultured or stimulated with EVs was assessed by quantitative real-time PCR. High Capacity cDNA Reverse Transcription Kit (Applied Biosystems) and the Power SYBR® Green PCR Master Mix (Applied Biosystems) were used as previously described [26]. Negative cDNA controls (no cDNA) were cycled in parallel with each run. Quantitative real-time polymerase chain reaction (qRT-PCR) was performed using a 96-well StepOne Real-Time System (Applied Biosystems). Sequence-specific oligonucleotide primers were purchased from MWG-Biotech AG (Ebersberg, Germany, www.mwg-biotech.com) and are shown in Table 1. Fold change in mRNA expression compared to control was determined as 2-ΔΔCt for all samples, using TBP as normalizer. The endogenous control in EVs was significantly different from that of their cells of origin. For this reason, miRNA comparisons between cells and EVs was not performed.

MicroRNA profiling by quantitative real-time PCR

Mature miRNA expression levels in EVs were analyzed as previously described [29,30]. The Applied Biosystems TaqMan® MicroRNA Assay Human Panel Early Access Kit (Life Technology) was used to profile 754 mature miRNAs by sequential steps of reverse transcription (Megaplex RT Pools; Life Technology) using an Applied Biosystems 7900H qRT-PCR instrument. The SDS software (version 2.3) was used to calculate raw CT values, automatic baseline, and threshold. Since a CT value of 35 represents single molecule template detection, CT values higher than 35 were considered to be below the detection level of the assay and excluded from the analyses.

To confirm the expression of MET-related miRNAs, screened by microarray analysis, miScript Reverse Transcription Kit and miScript SYBR Green PCR Kit (both from Qiagen) were used as previously described [22]. All samples were run in triplicate and 3 ng of cDNA were used for each reaction, as described by the manufacturer’s protocol (Qiagen). MiRNAs specific primers to hsa-miR-200a, 200b, 200c, 141 and 429 are listed in Table 2 and were all used in the same reaction. The small nucleolar RNA RNU-6B was used as reference control to normalize data. A 96-well StepOneTM Real Time System (Applied Biosystems) was used to perform qRT-PCR.

MicroRNA target prediction and pathway analysis

The web-based application DIANA-mirPath (version 2.0) was used to perform the enrichment analysis of predicted target genes by miRNAs in biological pathways. The algorithm microT-CDS was chosen to predict EVs-derived miRNA targets, using the default microT threshold of 0.8.

DIANA-mirPath performed an enrichment analysis of multiple miRNA target genes to all known KEGG pathways, as previously described [36,37]. The statistical significance value associated with the identified biological functions was calculated by the mirPath software (http://microrna.gr/mirpath). Biological pathways showing p-value less than 0.001 were considered as significantly enriched.

MSC transfection with miRNA mimics

MSCs were transiently transfected with miR-200a, miR-200b, miR-200c, miR-141 and miR-429 mimics (20 μM, MiScript miRNA mimics, Qiagen) using the HiPerFect Transfection Reagent (Qiagen), according to the manufacturer’s protocol. Briefly, MSCs were seeded into 6-well plates at a density of 10,000 cells/cm2. MiRNA mimics at a concentration of 20 nM were mixed with an appropriated volume of HiPerFect Transfection Reagent (Qiagen) and incubated at room temperature for 10 minutes. Allstars negative control siRNA (20 μM, Qiagen) was used as scrambled control. The transfection mix was added dropwise to the cells in FBS-depleted culture medium, in agreement with the manufacturer's instructions. After 24-hours of incubation, the transfection medium was removed, and cells were cultured in MSCBM for 7 days.

Luciferase reporter assays

The pEZX-MT05 luciferase reporter vectors containing the 3′-untranslated region (UTR) sequence of human cyclin D1 (CCND1, accession number NM_053056.2) and human insulin-like growth factor 1 receptor (IGF1R, accession number NM_000875.3) inserted downstream of the luciferase reporter gene were obtained from GeneCopoeia (Rockville, MD). For luciferase reporter assays, HEK 293T cells were seeded in 24-well plates in DMEM high glucose lacking antibiotics. Luciferase-3’UTR reporter constructs (0.8 μg) or the empty expression vector (negative control) were co-transfected with miR-200a, miR-200b, miR-200c, miR-141 and miR-429 mimics (0.5 μg, MiScript miRNA mimics, Qiagen) using Lipofectamine 2000 (Invitrogen) according to the manufacturer’s instructions. After 24 hours of transfection, medium was replaced by DMEM high glucose with 10% FBS. Twenty-four hours later, firefly and Renilla luciferase activities were measured in the culture medium of the same samples using the LucPair™ miR Duo-Luciferase Assay Kit, as previously described [38].

Statistical analysis

Statistical analysis was performed by using the t test. Statistical significance was set at P < 0.05.

Results

RPTECs induce epithelial commitment of MSCs

To investigate the effects of RPTECs on MSCs, human bone marrow-derived MSCs and RPTECs were co-cultured in not-contact conditions. After 7 days, mRNA levels of specific mesenchymal markers Twist (TWIST1), vimentin (VIM) and FOXC2 were significant reduced in MSCs (Fig 1A and 1E); moreover, MSCs expressed higher levels of the epithelial-specific marker cytokeratin 18 (KRT18), suggesting that MET occurred in MSCs (Fig 1B and 1H). Same results were observed when MSCs were incubated with TOT-CM (Fig 1A, 1B, 1D and 1G). To investigate the contribution of paracrine factors in epithelial differentiation of MSCs induced by RPTECs, MSCs were also incubated with CM or with purified EVs. Interestingly, after one week of incubation with CM, we did not observe any change in the expression of mesenchymal and epithelial markers in MSCs, suggesting that the contribution of soluble factors is not sufficient to induce the epithelial commitment of MSCs (Fig 1A and 1B). In MSCs stimulated with EVs, we observed a significant reduction in the expression of mesenchymal markers (Fig 1A and 1C) and an increase in the expression of the epithelial-specific marker KRT18, in a manner comparable with co-culture system (Fig 1B and 1F). These results indicate that EVs play a relevant role in inducing MET in MSCs.

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Fig 1. Analysis of mesenchymal and epithelial markers expression in MSCs treated for one week.

(A-B) Histograms showing relative expression (RQ) in respect to control cells (CTR, grey bars) of mesenchymal markers (A) and epithelial markers (B) in MSCs, after one week of co-culture with RPTECs (striped bars), or after stimulation with EVs (black bars) or RPTEC-derived conditioned medium (TOT-CM, dotted bars) or conditioned medium deprived of EVs (CM, white bars). Results are expressed as mean of six independent experiments performed in triplicate. Data were analysed via a Student’s t test (unpaired, 2-tailed); *P<0,05 versus CTR. (C-H) Representative micrographs showing the expression of vimentin (C, D, E) and cytokeratins (F, G, H) by MSCs stimulated with EVs (C-F), TOT-CM (D-G), or co-cultured with RPTECs (E-H). Nuclei were counterstained with Hoechst dye. Six independent experiments were performed with similar results. Original magnification: X630.

https://doi.org/10.1371/journal.pone.0159163.g001

Notably, the down-regulation of the expression of mesenchymal markers and the increase in cytokeratin 18 expression were also maintained after two weeks of stimulation with EVs (Fig 2A, 2B and 2C), TOT-CM (Fig 2A, 2B and 2D) and of co-culture with RPTECs (Fig 2A, 2B and 2E). A slight but significant increase in expression of the renal tubular-specific marker aminopeptidase A (ENPEP) was also observed in MSCs stimulated with EVs (Fig 2B and 2F), TOT-CM (Fig 2B and 2G). The early expression of ENPEP in MSCs co-cultured with RPTECs (Fig 1B) was also maintained after 14 days (Fig 2B and 2H), suggesting that the renal tubular commitment of MSCs was facilitated by a bidirectional exchange of paracrine factors between the two cell populations.

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Fig 2. Analysis of mesenchymal and epithelial markers expression in MSCs treated for two weeks.

(A-B) Histograms showing relative expression (RQ) in respect to control cells (CTR, grey bars) of mesenchymal markers (A) and epithelial markers (B) in MSCs, after two weeks of co-culture with RPTECs (striped bars), or after stimulation with EVs (black bars) or RPTEC-derived conditioned medium (TOT-CM, dotted bars). Results are expressed as mean of six independent experiments performed in triplicate. Data were analysed via a Student’s t test (unpaired, 2-tailed); *P<0.05 versus CTR. (C-H) Representative micrographs showing the expression of cytokeratin 18 (C, D, E) and aminopeptidase A (F, G, H) by MSCs stimulated with EVs (C-F), TOT-CM (D-G), or co-cultured with RPTECs (E-H). Nuclei were counterstained with Hoechst dye. Original magnification: X630. (I) Significant increased uptake of FITC-labeled albumin (BSA FITC) by MSC monolayers co-cultured with RPTECs, stimulated with EVs or with TOT-CM; *P<0.05 versus CTR. (J) Significant variation of TEER in MSC monolayers co-cultured with RPTECs, stimulated with EVs or with TOT-CM; *P<0.05 versus CTR.

https://doi.org/10.1371/journal.pone.0159163.g002

Human proximal tubular epithelial cells can effectively reabsorb albumin by receptor-mediated endocytosis [39]. To verify whether this tubular epithelial-specific function was induced by EVs in MSCs, we quantified fluorescently-labeled albumin uptake using cytofluorimetric analysis. MSCs stimulated with EVs, TOT-CM and co-cultured with RPTECs successfully incorporated FITC-labeled albumin (Fig 2I). Moreover, evaluation of TEER as an indicator of epithelial differentiation and integrity showed that EVs and TOT-CM induced a significant increase of TEER in MSCs (Fig 2J). Taken together, these results confirm that EVs can induce the epithelial commitment of MSCs.

Characterization of EVs and incorporation into MSCs

To better clarify the mechanisms underlying the epithelial commitment induced by RPTECs on MSCs, we evaluated the capacity of EVs to be incorporated into MSCs and characterized EVs for the presence of specific proteins and mRNAs. Starting from 6 hours of incubation, labeled EVs were internalized by MSCs, with a progressive compartmentalization of EVs inside the cell at 15 and 24 hours of incubation (Fig 3).

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Fig 3. Incorporation of EVs in MSCs.

Representative micrographs of internalization by MSCs of EVs stained with Vybrant Dil (red) at 37°C for 6 hours (A), 15 hours (B), 24 hours (C) observed by Confocal microscopy. Z-stack was performed to verify the effective internalization of EVs. Nuclei were counterstained with Hoechst dye. Three experiments were performed with similar results. Original magnification: X630.

https://doi.org/10.1371/journal.pone.0159163.g003

Cytofluorimetric analysis showed that EVs carried several surface adhesion molecules also expressed on the plasma membrane of RPTECs, such as CD24, CD29, CD44, CD73, CD146, alpha-5 integrin (CD49e), alpha-6 integrin (CD49f), HLA1 and EpCAM. EVs also expressed classical exosomal markers CD63, CD81 and CD107a (LAMP1) (Fig 4A). Moreover, we found that EVs shuttled both epithelial-specific proteins and mRNA, such as cytokeratins, and the tubular-specific marker ENPEP (Fig 4B and Table 3).

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Fig 4. Characterization of EVs protein expression.

(A) Characterization of EVs by cytofluorimetric analysis. Representative FACS analyses of EVs showing the expression of CD24, CD29, CD44, alpha-5 integrin (CD49e), alpha-6 integrin (CD49f), CD73, CD146, EpCAM, and HLA-class I surface molecules and classic exosomal markers CD63, CD81, CD107 (thick lines). Dotted lines indicate the isotypic controls. Three different EV preparations were analyzed with similar results. (B) Representative western blot analysis on RPTEC cells and EVs. Three different experiments were performed with similar results.

https://doi.org/10.1371/journal.pone.0159163.g004

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Table 3. Analysis of epithelial-specific mRNAs expression by RPTEC cells and EVs.

Results are expressed as mean ± SD of three independent experiments.

https://doi.org/10.1371/journal.pone.0159163.t003

Nanosight analysis revealed that the average size of EVs was 185 nm with a mode of 163 nm and a standard deviation of 84 nm (Fig 5A). EVs presence was also confirmed in TOT-CM, with an average size of 162 nm, a mode of 141 nm and a standard deviation of 84 nm (Fig 5B). After RPTEC supernatant ultracentrifugation, EVs concentration was highly reduced in CM (Fig 5B).

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Fig 5. Characterization of EVs size and RNA content.

(A-B) Representative EV size analysis by direct measurement with NTA, in EVs (A) and in RPTEC-derived conditioned medium with (TOT-CM) or without EVs (CM) (B) by direct measurement with NTA, showing the difference of EV concentration before and after EV depletion. (C) Representative Bioanalyzer profiles, showing the size distribution of total RNA extracted from EVs and cells. The first peak (left side of each panel) represents an internal standard. Whereas the two peaks of ribosomal RNA 18S and 28S were detectable in cells, they were barely detectable in the corresponding EVs. Unlike the cells of origin, EVs exhibited a relevant peak of small RNAs. RNA Integrity Number (RIN) is shown for both cells and EVs. (D) Representative bioanalyzer profile of small RNAs performed on EVs, showing an enrichment of the miRNA fraction (range: 33–36%) in respect to the cells of origin (range: 4–7%). Three different samples tested in triplicate were analyzed for both EVs and cells with similar results.

https://doi.org/10.1371/journal.pone.0159163.g005

MicroRNA profiling in EVs and comparative pathway analyses

We verified the quality of EVs-derived RNA and the presence of small RNAs, with a bioanalyzer profile on total RNA from EVs and their cell of origin. EVs contained a broad range of RNA sizes, with a RNA Integrity Number (RIN) of 7.30 out of 10 (Fig 5C). A more comprehensive analysis using a bioanalyzer kit specific for small RNAs showed a relevant peak characteristic of small RNA classes inside EVs, with an enrichment of miRNAs around 36% (Fig 5D). RNA extracted from EVs was profiled for 754 known human mature miRNAs. We found 237 miRNAs expressed (S1 Table). Among them, we found a subset of five miRNAs (miR-200a, miR-200b, miR-200c, miR-141 and miR-429) that belong to miR-200 family, known to be involved in EMT [40,41].

In order to examine which biological pathways may be involved in the regulation of the epithelial commitment of target cells, we applied the software DIANA MirPath on the 65 most expressed miRNAs derived from EVs. We performed an enrichment analysis of predictive miRNA target genes included in KEGG database and we found that 63 KEGG biological processes were significantly enriched (p<0.001, FDR corrected) (S2 Table). Twenty miRNAs found in EVs revealed a strong association to several biological pathways that are known to modulate EMT (Table 4).

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Table 4. MiRNAs shuttled by EVs and associated to EMT-related KEGG pathways.

Results are expressed as mean ± SD of three independent experiments.

https://doi.org/10.1371/journal.pone.0159163.t004

Our analysis showed that the predicted target genes of these miRNAs are principally involved into the following EMT and MET-associated pathways: ECM-receptor interaction, Wnt pathway, gap junction, transcriptional misregulation in cancer, TGF-beta pathway, pathways in cancer, MAPK signaling pathway, p53 signaling pathway, focal adhesion, PI3K-Akt signaling pathway, regulation of actin cytoskeleton (Table 5) [11,4245]. Fig 6 provides a graphical representation of the most significantly enriched pathways modulated by the 20 miRNAs that we selected from our analysis.

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Fig 6. Heat map showing miRNAs versus pathways.

Using the option union of pathways, DIANA MirPath provided a graphical overview of pathways enriched by the 20 selected EVs-derived miRNAs. Darker colors represent lower significance values. MET-related pathways (highlighted by the circle line) are targeted by the selected miRNAs with a very low p-value (p<10−7, FDR corrected). The attached dendrograms illustrate hierarchical clustering results for miRNAs and pathways. MiRNAs that show similar pathway targeting patterns were clustered together. An analogous clustering was also performed for the biological pathways.

https://doi.org/10.1371/journal.pone.0159163.g006

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Table 5. Biologic pathways enriched by 20 selected miRNAs found in EVs, that contain EMT-related genes.

https://doi.org/10.1371/journal.pone.0159163.t005

We selected two miRNA targets from our predictive analysis, CCND1 and IGF-1R, and examined their expression in MSCs after one week of incubation with EVs or TOT-CM. In both conditions, we observed a reduction in the expression of CCND1 and IGF-1R in MSCs, that could be attributed to miRNA-mediated inhibitory effects (Fig 7). These data suggest that EVs may prompt an epithelial commitment in target cells, by the delivery of specific miRNAs involved in MET-related pathways.

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Fig 7. Analysis of miRNA predictive target genes in MSCs stimulated with EVs.

Histograms showing relative expression (RQ) of miRNA predictive target genes in MSCs, after one (A) and two weeks (B) of stimulation with EVs (black bars), or RPTEC-derived conditioned medium (TOT-CM, dotted bars), in respect to control cells (CTR, grey bars). Results are expressed as mean of six independent experiments performed in triplicate. Data were analyzed via a Student’s t test (unpaired, 2-tailed); *P<0.05 versus CTR.

https://doi.org/10.1371/journal.pone.0159163.g007

Role of the miR-200 family in the epithelial commitment of MSCs

We employed qRT-PCR to validate the expression levels of the five miRNAs belonging to miR-200 family, selected from the miRNA array. We showed that all these five miRNAs were strongly expressed in EVs and we selected them to study their possible role in MET induction in MSCs. A mixture of mimics was used to increase the expression of miR-200a, miR-200b, miR-200c, miR-141 and miR-429 in MSCs. After 1 week of transfection, MSCs showed lower levels of MET markers VIM and fibronectin 1 (FN1) (Fig 8A), and higher levels of epithelial marker KRT18 and tubular marker ENPEP (Fig 8B). Moreover, MSCs transfection with miR-200 mimics reduced the expression of two miRNA targets from our predictive analysis, CCND1 and IGF-1R (Fig 8C).

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Fig 8. Analysis of mesenchymal and epithelial markers expression in MSCs transfected with miR-200 mimics.

Histograms showing relative expression (RQ) of mesenchymal markers (A), epithelial markers (B) and miRNA predictive target genes (C) in MSCs, after one week of transfection with miR-200 mimics (black bars), or with a control miRNA (scramble, white bars), in respect to control cells (CTR, grey bars). Results are expressed as mean of three independent experiments performed in triplicate. Data were analysed via a Student’s t test (unpaired, 2-tailed); *P<0.05 versus CTR. (D) Luciferase expression in HEK 293T cells following co-transfection of CCND1 or IGF1R 3’UTR reporter constructs and miR-200 family mimics for 24 hours. Firefly luciferase expression is normalized to Renilla luciferase for each gene-specific 3’UTR and presented as a percentage of the luciferase activity variation in respect to the same cells co-transfected with a negative control vector (CTR). Values are expressed as mean of three independent experiments; *P<0.05 versus CTR.

https://doi.org/10.1371/journal.pone.0159163.g008

To assess whether miR-200 family can effectively repress translation through binding to CCND1 and IGF1R 3’UTR, we performed luciferase reporter assay. MiR-200 family mimics were co-transfected in HEK 293T cells with the luciferase reporter construct pEZX-MT05 containing the human CCND1 or IGF1R 3’UTR immediately following the luciferase coding sequence. As a result, miR-200 family induced a 90% reduction of luciferase activity in transfected cells.

Taken together, these results suggest that the miR-200 family carried by EVs can induce MET in MSCs by binding to the 3’UTR sequences of predicted target genes, like CCND1 and IGF1R (Fig 8D).

Discussion

The mechanism of cell communication mediated by EVs allows exchange of proteins and genetic information between cells, as EVs may transfer mRNAs, long non coding RNAs (lncRNAs) and miRNAs to target cells [18,20,4648]. The epithelial commitment of bone marrow-derived cells induced by EVs derived from differentiated tissues has been demonstrated by Quesenberry’s group [49]. They showed that EV-mediated transfer of proteins and genetic information from lung injured cells to bone marrow-derived cells may reprogram marrow cell phenotype to acquire lung epithelial-specific markers [19,20]. Moreover, EVs derived from prostate or lung cancer cells and EVs derived from lung injured cells were also shown to trigger stable epigenetic changes in marrow cells, activating the expression of prostate- or lung-specific genes [50,51], following internalization of EVs into target cells [52]. Taken together, these results indicate that EVs collected from differentiated injured tissues can effectively induce epigenetic modifications of marrow cells, that acquire phenotypic characteristics of the tissue of origin.

Previous studies have shown that tubular epithelial cells and their conditioned medium may induce an epithelial transition of MSCs [14]. In the present study, we have demonstrated that EVs released by RPTECs are the main mediators of the epithelial differentiation of bone marrow-derived MSCs. In fact, we noticed that RPTEC-derived conditioned medium depleted of EVs was no longer able to induce MET in MSCs. In particular, after one week of incubation of MSCs with EVs, we observed the decreased expression of TWIST1, FOXC2, known to repress epithelial genes expression [53,54], and of vimentin, a protein involved in cellular adhesion and migration [55,56]. Moreover, after two weeks of MSC stimulation with EVs, we observed the increased expression of epithelial marker cytokeratin 18, which contributes to maintenance of epithelial cell polarity and plays an important role in cellular adhesion and cell-to-cell interactions [5759], and a slight increase in the expression of aminopeptidase A. This zinc-dependent metalloproteinase is typically expressed in the brush border membrane of renal proximal tubule cells and it is known to be involved into the removal of N-terminal acid aminoacidic remainings from different peptides, for example angiotensin II [60,61]. Taken together, these results indicate an epithelial differentiation of MSCs induced by EVs.

To understand the mechanism of epithelial commitment of MSCs induced by EVs, we characterized EV protein and RNA content. We found that EVs contained epithelial-specific proteins and transcripts that after delivering to target cells may be responsible for the early epithelial commitment of MSCs. The persistence of KRT18 expression in MSCs after 14 days of stimulation with EVs suggests that epigenetic changes contributed to maintain MSCs epithelial commitment. The long-term modification in MSC transcriptome was probably due to epigenetic changes that follow the transfer of non-coding RNAs, such as miRNAs [62]. Recently, the EVs-mediated transfer of miRNAs has been observed between differentiated normal cells [21,63], between MSCs and differentiated cells [6466], between MSCs and cancer cells [6769] and inside the tumor microenvironment [7072].

To investigate the miRNA content of EVs, we profiled their RNA for 754 known human mature miRNAs and we identified 20 miRNAs with a strong association to EMT pathways. In particular, we detected the expression of some miRNAs belonging to miR-200 family. Recent studies on tumor cells [7376] have demonstrated that miR-200 family miRNAs (miR-200a, miR-200b, miR-200c, miR-141, miR-429) are involved in EMT. In fact, mature miR-200 family miRNAs promote E-cadherin expression with the acquisition of an epithelial cell phenotype via post-transcriptional repression of zinc finger E-box binding transcription factor 1 and 2 (ZEB1 and ZEB2) [77]. During EMT, ZEB1 and ZEB2 over-expression leads to transcriptional repression of E-cadherin, promoting a mesenchymal cell phenotype. This process may be reversible, since an increase in miR-200 family miRNAs expression initiates MET, restoring E-cadherin expression and promoting an epithelial phenotype [77].

Since miR-200 family miRNAs are shuttled by EVs, we investigated the effects of these miRNAs in MSCs and their possible contribution to MET. After one week of transfection of bone marrow derived-MSCs with 5 synthetic miR-200 mimics, we observed a reduction in the expression of VIM and FN1, which is another mesenchymal marker involved in cell adhesion, cell migration, cell growth and cell differentiation [78]. Moreover, we observed an increased expression of ENPEP, indicating that the miR-200 miRNAs can induce the epithelial commitment of MSCs. These data suggest that EVs may contribute to the epithelial commitment of MSCs by transferring a small subset of miRNAs that belong to the miR-200 family.

Furthermore, in order to validate the results of our predictive analysis on EV-derived miRNAs, we randomly selected cyclin D1 (CCND1) and insulin growth factor-1 receptor (IGF1R), from all predictive miRNA target genes.

CCND1 encodes a regulatory subunit of the cyclin-dependent kinase 4 (CDK4) and of the cyclin-dependent kinase 6 (CDK6), whose activity is required for cell cycle G1/S transition [79]. CCND1 is involved in cell proliferation, survival, invasion, metastasis formation and its over-expression is linked to tumorigenesis [80,81]. Recent studies have demonstrated that CCND1 activation can induce EMT in tumor cells, such as ovarian cancer [82], breast cancer [83], esophageal cancer [84] and epidermoid carcinoma cells [85]. In particular, Su et al. [84] have shown that the inhibition of CCND1 down-regulates the expression of other mesenchymal markers and reverses EMT in esophageal cancer cells.

IGF1R is a trans-membrane receptor tyrosine kinase which binds to its ligand IGF1, leading to activation of the PI3K-Akt pathway and the Erk-MAPK pathway. Previous studies have shown that IGF1R activation can induce EMT in prostate cancer [86], breast cancer [87,88], mammary epithelial cells [89] and lung cancer cells [34,90]. Nurwidya et al. [35] found that inhibition of IGF1R reversed hypoxia-induced EMT. Zhou et al. [90] reported that IGF1R activation induces EMT in lung cancer cells by up-regulating the expression of Snail and promoting beta-catenin translocation from the cell membrane into the nucleus, which, in turn, down-regulates E-cadherin expression.

We evaluated the expression of CCND1 and IGF1R in MSCs after incubation with EVs or TOT-CM and after cell transfection with miR-200 mimics. We showed that both EVs and miR-200 family miRNAs can effectively reduce CCND1 and IGF1R expression in MSCs. These results confirmed that CCND1 and IGF1R down-regulation is indicative of MET. Luciferase reporter assay has proved that both CCND1 and IGF1R are target genes of EV-delivered miRNAs, thus validating the results of our miRNA predictive analysis.

In conclusion, EVs released from tubular epithelial cells may modify the phenotype of MSCs by inducing an epithelial commitment that may contribute to the regenerative potential of MSCs. Whether this phenomenon occurs in vivo remains to be defined.

Supporting Information

S1 Fig. Characterization of human bone marrow-derived MSCs.

A-B) Representative micrographs showing the expression of vimentin (A) and cytokeratins (B) by MSCs. Nuclei were counterstained with Hoechst dye. Three independent experiments were performed with similar results. Original magnification: X630. C) Representative FACS analyses of MSCs showing the expression of CD29, CD44, CD73, CD90 and CD105 surface molecules (blue area). The expression of EpCAM was not detected. Green lines indicate the isotypic controls. Six different MSCs preparations were analyzed with similar results.

https://doi.org/10.1371/journal.pone.0159163.s001

(TIF)

S2 Fig. Characterization of human renal tubular cells (RPTECs).

A-B) Representative micrographs showing the expression of vimentin (A) and cytokeratins (B) by MSCs. Nuclei were counterstained with Hoechst dye. Three independent experiments were performed with similar results. Original magnification: X630. C) Representative FACS analyses of RPTECs showing the expression of CD24, CD29, CD44, alpha-5 integrin (CD49e), alpha-6 integrin (CD49f), CD73, CD146, EpCAM, and HLA-class I surface molecules (blue area). The expression of VEGF receptor II (KDR), CD45 and CD105 was not detected. Dotted lines indicate the isotypic controls. Six different RPTECs preparations were analyzed with similar results.

https://doi.org/10.1371/journal.pone.0159163.s002

(TIF)

S1 Table. List of 237 miRNAs found in EVs.

Results are expressed as mean ± SD of three independent experiments.

https://doi.org/10.1371/journal.pone.0159163.s003

(DOCX)

S2 Table. List of KEGG biological pathways significantly enriched (p<0.001, FDR corrected) by miRNAs found in EVs.

https://doi.org/10.1371/journal.pone.0159163.s004

(DOCX)

Author Contributions

Conceived and designed the experiments: G. Chiabotto SB G. Camussi. Performed the experiments: G. Chiabotto SB. Analyzed the data: G. Chiabotto SB FC G. Camussi. Contributed reagents/materials/analysis tools: FC G. Camussi. Wrote the paper: G. Chiabotto SB FC G. Camussi.

References

  1. 1. Singaravelu K, Padanilam BJ. In vitro differentiation of MSC into cells with a renal tubular epithelial-like phenotype. Ren Fail. 2009;31(6):492–502. pmid:19839827
  2. 2. Baer PC, Bereiter-Hahn J, Missler C, Brzoska M, Schubert R, Gauer S, et al. Conditioned medium from renal tubular epithelial cells initiates differentiation of human mesenchymal stem cells. Cell Prolif. 2009 Feb;42(1):29–37. pmid:19143761
  3. 3. Wan JX, Zou ZH, You DY, Cui J, Pan YB. Bone marrow-derived mesenchymal stem cells differentiation into tubular epithelial-like cells in vitro. Cell Biochem Funct. 2012 Mar;30(2):129–38. pmid:22125055
  4. 4. Papadimou E, Morigi M, Iatropoulos P, Xinaris C, Tomasoni S, Benedetti V, et al. Direct reprogramming of human bone marrow stromal cells into functional renal cells using cell-free extracts. Stem Cell Reports. 2015 Apr 14;4(4):685–98. pmid:25754206
  5. 5. Fanni D, Fanos V, Monga G, Gerosa C, Nemolato S, Locci A, et al. MUC1 in mesenchymal-to-epithelial transition during human nephrogenesis: changing the fate of renal progenitor/stem cells? J Matern Fetal Neonatal Med. 2011 Oct;24 Suppl 2:63–6. pmid:21966898
  6. 6. Kanazawa T, Ichii O, Otsuka S, Namiki Y, Hashimoto Y, Kon Y. Hepatocyte nuclear factor 4 alpha is associated with mesenchymal-epithelial transition in developing kidneys of C57BL/6 mice. J Vet Med Sci. 2011 May;73(5):601–7. pmid:21186337
  7. 7. Kalluri R, Neilson EG. Epithelial-mesenchymal transition and its implications for fibrosis. J Clin Invest. 2003 Dec;112(12):1776–84. pmid:14679171
  8. 8. Lee JM, Dedhar S, Kalluri R, Thompson EW. The epithelial-mesenchymal transition: new insights in signaling, development, and disease. J Cell Biol. 2006 Mar 27;172(7):973–81. pmid:16567498
  9. 9. Guarino M. Epithelial-mesenchymal transition and tumour invasion. Int J Biochem Cell Biol. 2007;39(12):2153–60. pmid:17825600
  10. 10. Yang J, Weinberg RA. Epithelial-mesenchymal transition: at the crossroads of development and tumor metastasis. Dev Cell. 2008 Jun;14(6):818–29. pmid:18539112
  11. 11. Kalluri R, Weinberg RA. The basics of epithelial-mesenchymal transition. J Clin Invest. 2009 Jun;119(6):1420–8. pmid:19487818
  12. 12. Thiery JP, Acloque H, Huang RY, Nieto MA. Epithelial-mesenchymal transitions in development and disease. Cell. 2009 Nov 25;139(5):871–90. pmid:19945376
  13. 13. Nieto MA. The ins and outs of the epithelial to mesenchymal transition in health and disease. Annu Rev Cell Dev Biol. 2011;27:347–76. pmid:21740232
  14. 14. Lipschutz JH. Molecular development of the kidney: a review of the results of gene disruption studies. Am J Kidney Dis. 1998 Mar;31(3):383–97. pmid:9506676
  15. 15. Rothenpieler UW, Dressler GR. Pax-2 is required for mesenchyme-to-epithelium conversion during kidney development. Development. 1993 Nov;119(3):711–20. pmid:8187639
  16. 16. Hogan BL, Kolodziej PA. Organogenesis: molecular mechanisms of tubulogenesis. Nat Rev Genet. 2002 Jul;3(7):513–23. pmid:12094229
  17. 17. Ratajczak J, Wysoczynski M, Hayek F, Janowska-Wieczorek A, Ratajczak MZ. Membrane-derived microvesicles: important and underappreciated mediators of cell-to-cell communication. Leukemia. 2006 Sep;20(9):1487–95. pmid:16791265
  18. 18. Ratajczak J, Miekus K, Kucia M, Zhang J, Reca R, Dvorak P, et al. Embryonic stem cell-derived microvesicles reprogram hematopoietic progenitors: evidence for horizontal transfer of mRNA and protein delivery. Leukemia. 2006 May;20(5):847–56. pmid:16453000
  19. 19. Aliotta JM, Sanchez-Guijo FM, Dooner GJ, Johnson KW, Dooner MS, Greer KA, et al. Alteration of marrow cell gene expression, protein production, and engraftment into lung by lung-derived microvesicles: a novel mechanism for phenotype modulation. Stem Cells. 2007 Sep;25(9):2245–56. pmid:17556595
  20. 20. Aliotta JM, Pereira M, Johnson KW, de Paz N, Dooner MS, Puente N, et al. Microvesicle entry into marrow cells mediates tissue-specific changes in mRNA by direct delivery of mRNA and induction of transcription. Exp Hematol. 2010 Mar;38(3):233–45. pmid:20079801
  21. 21. Valadi H, Ekström K, Bossios A, Sjöstrand M, Lee JJ, Lötvall JO. Exosome-mediated transfer of mRNAs and microRNAs is a novel mechanism of genetic exchange between cells. Nat Cell Biol. 2007 Jun;9(6):654–9. pmid:17486113
  22. 22. Collino F, Deregibus MC, Bruno S, Sterpone L, Aghemo G, Viltono L, et al. Microvesicles Derived from Adult Human Bone Marrow and Tissue Specific Mesenchymal Stem Cells Shuttle Selected Pattern of miRNAs. PLoS One. 2010 Jul 27;5(7):e11803. pmid:20668554
  23. 23. Penfornis P, Vallabhaneni KC, Whitt J, Pochampally R. Extracellular vesicles as carriers of microRNA, proteins and lipids in tumor microenvironment. Int J Cancer. 2016 Jan 1;138(1):14–21. pmid:25559768
  24. 24. Bartel DP. MicroRNAs: genomics, biogenesis, mechanism, and function. Cell. 2004 Jan 23;116(2):281–97. pmid:14744438
  25. 25. Lagos-Quintana M, Rauhut R, Lendeckel W, Tuschl T. Identification of novel genes coding for small expressed RNAs. Science. 2001 Oct 26;294(5543):853–8. pmid:11679670
  26. 26. Bruno S, Grange C, Deregibus MC, Calogero RA, Saviozzi S, Collino F et al. Mesenchymal stem cell-derived microvesicles protect against acute tubular injury. J Am Soc Nephrol. 2009 May;20(5):1053–67. pmid:19389847
  27. 27. Bruno S, Grange C, Collino F, Deregibus MC, Cantaluppi V, Biancone L, et al. Microvesicles Derived from Mesenchymal Stem Cells Enhance Survival in a Lethal Model of Acute Kidney Injury. PLoS One. 2012;7(3):e33115. pmid:22431999
  28. 28. Théry C, Amigorena S, Raposo G, Clayton A. Isolation and characterization of exosomes from cell culture supernatants and biological fluids. Curr Protoc Cell Biol. 2006 Apr;Chapter 3:Unit 3.22.
  29. 29. Collino F, Bruno S, Incarnato D, Dettori D, Neri F, Provero P, et al. AKI Recovery Induced by Mesenchymal Stromal Cell-Derived Extracellular Vesicles Carrying MicroRNAs. J Am Soc Nephrol. 2015 Oct;26(10):2349–60. pmid:25901032
  30. 30. Lindoso RS, Collino F, Bruno S, Araujo DS, Sant'Anna JF, Tetta C, et al. Extracellular vesicles released from mesenchymal stromal cells modulate miRNA in renal tubular cells and inhibit ATP depletion injury. Stem Cells Dev. 2014 Aug 1;23(15):1809–19. pmid:24669934
  31. 31. Grange C, Tapparo M, Bruno S, Chatterjee D, Quesenberry PJ, Tetta C, et al. Biodistribution of mesenchymal stem cell-derived extracellular vesicles in a model of acute kidney injury monitored by optical imaging. Int J Mol Med. 2014 May;33(5):1055–63. pmid:24573178
  32. 32. Jang KJ, Mehr AP, Hamilton GA, McPartlin LA, Chung S, Suh KY, et al. Human kidney proximal tubule-on-a-chip for drug transport and nephrotoxicity assessment. Integr Biol (Camb). 2013 Sep;5(9):1119–29.
  33. 33. Wessel D, Flügge UI. A method for the quantitative recovery of protein in dilute solution in the presence of detergents and lipids. Anal Biochem. 1984 Apr;138(1):141–3. pmid:6731838
  34. 34. Dimuccio V, Ranghino A, Praticò Barbato L, Fop F, Biancone L, Camussi G, et al. Urinary CD133+ extracellular vesicles are decreased in kidney transplanted patients with slow graft function and vascular damage. PLoS One. 2014 Aug 6;9(8):e104490. pmid:25100147
  35. 35. Nurwidya F, Takahashi F, Kobayashi I, Murakami A, Kato M, Minakata K, et al. Treatment with insulin-like growth factor 1 receptor inhibitor reverses hypoxia-induced epithelial-mesenchymal transition in non-small cell lung cancer. Biochem Biophys Res Commun. 2014 Dec 12;455(3–4):332–8. pmid:25446090
  36. 36. Vlachos IS, Kostoulas N, Vergoulis T, Georgakilas G, Reczko M, Maragkakis M, et al. DIANA miRPath v.2.0: investigating the combinatorial effect of microRNAs in pathways. Nucleic Acids Res. 2012 Jul;40(Web Server issue):W498–504. pmid:22649059
  37. 37. Xu JF, Yang GH, Pan XH, Zhang SJ, Zhao C, Qiu BS, et al. Altered microRNA expression profile in exosomes during osteogenic differentiation of human bone marrow-derived mesenchymal stem cells. PLoS One. 2014 Dec 11;9(12):e114627. pmid:25503309
  38. 38. Hupkes M, Sotoca AM, Hendriks JM, van Zoelen EJ, Dechering KJ. MicroRNA miR-378 promotes BMP2-induced osteogenic differentiation of mesenchymal progenitor cells. BMC Mol Biol. 2014 Jan 27;15:1. pmid:24467925
  39. 39. Birn H, Christensen EI. Renal albumin absorption in physiology and pathology. Kidney Int. 2006 Feb;69(3):440–9. pmid:16514429
  40. 40. Korpal M, Kang Y. The emerging role of miR-200 family of microRNAs in epithelial-mesenchymal transition and cancer metastasis. RNA Biol. 2008 Jul-Sep;5(3):115–9. pmid:19182522
  41. 41. Mongroo PS, Rustgi AK. The role of the miR-200 family in epithelial-mesenchymal transition. Cancer Biol Ther. 2010 Aug 1;10(3):219–22. pmid:20592490
  42. 42. Campanaro S, Picelli S, Torregrossa R, Colluto L, Ceol M, Del Prete D, et al. Genes involved in TGF beta1-driven epithelial-mesenchymal transition of renal epithelial cells are topologically related in the human interactome map. BMC Genomics. 2007 Oct 22;8:383. pmid:17953753
  43. 43. Moustakas A, Heldin CH. Signaling networks guiding epithelial-mesenchymal transitions during embryogenesis and cancer progression. Cancer Sci. 2007 Oct;98(10):1512–20. pmid:17645776
  44. 44. Katoh Y, Katoh M. Hedgehog signaling, epithelial-to-mesenchymal transition and miRNA (review). Int J Mol Med. 2008 Sep;22(3):271–5. pmid:18698484
  45. 45. Liu X, Yun F, Shi L, Li ZH, Luo NR, Jia YF. Roles of Signaling Pathways in the Ep,thelial-Mesenchymal Transition in Cancer. Asian Pac J Cancer Prev. 2015;16(15):6201–6. pmid:26434817
  46. 46. Chen X, Liang H, Zhang J, Zen K, Zhang CY. Secreted microRNAs: a new form of intercellular communication. Trends Cell Biol. 2012 Mar;22(3):125–32. pmid:22260888
  47. 47. Gallo A, Tandon M, Alevizos I, Illei GG. The majority of microRNAs detectable in serum and saliva is concentrated in exosomes. PLoS One. 2012;7(3):e30679. pmid:22427800
  48. 48. Raposo G, Stoorvogel W. Extracellular vesicles: exosomes, microvesicles, and friends. J Cell Biol. 2013 Feb 18;200(4):373–83. pmid:23420871
  49. 49. Quesenberry PJ, Aliotta JM. Cellular phenotype switching and microvesicles. Adv Drug Deliv Rev. 2010 Sep 30;62(12):1141–8. pmid:20558219
  50. 50. Renzulli JF 2nd, Del Tatto M, Dooner G, Aliotta J, Goldstein L, Dooner M, et al. Microvesicle induction of prostate specific gene expression in normal human bone marrow cells. J Urol. 2010 Nov;184(5):2165–71. pmid:20850816
  51. 51. Del Tatto M, Ng T, Aliotta JM, Colvin GA, Dooner MS, Berz D, et al. Marrow cell genetic phenotype change induced by human lung cancer cells. Exp Hematol. 2011 Nov;39(11):1072–80. pmid:21864488
  52. 52. Aliotta JM, Pereira M, Sears EH, Dooner MS, Wen S, Goldberg LR, et al., Lung-derived exosome uptake into and epigenetic modulation of marrow progenitor/stem and differentiated cells. J Extracell Vesicles. 2015 Sep 16;4:26166. pmid:26385657
  53. 53. Yang J, Mani SA, Donaher JL, Ramaswamy S, Itzykson RA, Come C, et al. Twist, a master regulator of morphogenesis, plays an essential role in tumor metastasis. Cell. 2004 Jun 25;117(7):927–39. pmid:15210113
  54. 54. Mani SA, Yang J, Brooks M, Schwaninger G, Zhou A, Miura N, et al. Mesenchyme Forkhead 1 (FOXC2) plays a key role in metastasis and is associated with aggressive basal-like breast cancers. Proc Natl Acad Sci U S A. 2007 Jun 12;104(24):10069–74. pmid:17537911
  55. 55. Eckes B, Dogic D, Colucci-Guyon E, Wang N, Maniotis A, Ingber D, et al. Impaired mechanical stability, migration and contractile capacity in vimentin-deficient fibroblasts. J Cell Sci. 1998 Jul;111 (Pt 13):1897–907. pmid:9625752
  56. 56. Ivaska J, Pallari HM, Nevo J, Eriksson JE. Novel functions of vimentin in cell adhesion, migration, and signaling. Exp Cell Res. 2007 Jun 10;313(10):2050–62. pmid:17512929
  57. 57. Chu PG, Weiss LM. Keratin expression in human tissues and neoplasms. Histopathology. 2002 May;40(5):403–39. pmid:12010363
  58. 58. Owens DW, Lane EB. The quest for the function of simple epithelial keratins. Bioessays. 2003 Aug;25(8):748–58. pmid:12879445
  59. 59. Messai Y, Noman MZ, Derouiche A, Kourda N, Akalay I, Hasmim M, et al. Cytokeratin 18 expression pattern correlates with renal cell carcinoma progression: relationship with Snail. Int J Oncol. 2010 May;36(5):1145–54. pmid:20372788
  60. 60. Wang J, Cooper MD. Histidine residue in the zinc-binding motif of aminopeptidase A is critical for enzymatic activity. Proc Natl Acad Sci U S A. 1993 Feb 15;90(4):1222–6. pmid:8433982
  61. 61. Goto Y, Hattori A, Ishii Y, Mizutani S, Tsujimoto M. Enzymatic properties of human aminopeptidase A. Regulation of its enzymatic activity by calcium and angiotensin IV. J Biol Chem. 2006; 281: 23503–13. pmid:16790432
  62. 62. Aliotta JM, Pereira M, Li M, Amaral A, Sorokina A, Dooner MS, et al. Stable cell fate changes in marrow cells induced by lung-derived microvesicles. J Extracell Vesicles. 2012 Apr 16;1.
  63. 63. Njock MS, Cheng HS, Dang LT, Nazari-Jahantigh M, Lau AC, Boudreau E, et al. Endothelial cells suppress monocyte activation through secretion of extracellular vesicles containing antiinflammatory microRNAs. Blood. 2015 May 14;125(20):3202–12. pmid:25838349
  64. 64. Yuan A, Farber EL, Rapoport AL, Tejada D, Deniskin R, Akhmedov NB, et al. Transfer of microRNAs by embryonic stem cell microvesicles. PLoS One. 2009;4(3):e4722. pmid:19266099
  65. 65. Xin H, Li Y, Buller B, Katakowski M, Zhang Y, Wang X, et al. Exosome-mediated transfer of miR-133b from multipotent mesenchymal stromal cells to neural cells contributes to neurite outgrowth. Stem Cells. 2012 Jul;30(7):1556–64. pmid:22605481
  66. 66. Martin PJ, Haren N, Ghali O, Clabaut A, Chauveau C, Hardouin P, et al. Adipogenic RNAs are transferred in osteoblasts via bone marrow adipocytes-derived extracellular vesicles (EVs). BMC Cell Biol. 2015 Mar 18;16:10. pmid:25887582
  67. 67. Lee JK, Park SR, Jung BK, Jeon YK, Lee YS, Kim MK, et al. Exosomes derived from mesenchymal stem cells suppress angiogenesis by down-regulating VEGF expression in breast cancer cells. PLoS One. 2013 Dec 31;8(12):e84256. pmid:24391924
  68. 68. Katakowski M, Buller B, Zheng X, Lu Y, Rogers T, Osobamiro O, et al. Exosomes from marrow stromal cells expressing miR-146b inhibit glioma growth. Cancer Lett. 2013 Jul 10;335(1):201–4. pmid:23419525
  69. 69. Ono M, Kosaka N, Tominaga N, Yoshioka Y, Takeshita F, Takahashi RU, et al. Exosomes from bone marrow mesenchymal stem cells contain a microRNA that promotes dormancy in metastatic breast cancer cells. Sci Signal. 2014 Jul 1;7(332):ra63. pmid:24985346
  70. 70. Singh R, Pochampally R, Watabe K, Lu Z, Mo YY. Exosome-mediated transfer of miR-10b promotes cell invasion in breast cancer. Mol Cancer. 2014 Nov 26;13:256. pmid:25428807
  71. 71. Neviani P, Fabbri M. Exosomic microRNAs in the Tumor Microenvironment. Front Med (Lausanne). 2015 Jul 22;2:47.
  72. 72. Ridder K, Sevko A, Heide J, Dams M, Rupp AK, Macas J, et al. Extracellular vesicle-mediated transfer of functional RNA in the tumor microenvironment. Oncoimmunology. 2015 Mar 19;4(6):e1008371. pmid:26155418
  73. 73. Korpal M, Lee ES, Hu G, Kang Y. The miR-200 family inhibits epithelial-mesenchymal transition and cancer cell migration by direct targeting of E-cadherin transcriptional repressors ZEB1 and ZEB2. J Biol Chem. 2008 May 30;283(22):14910–4. pmid:18411277
  74. 74. Park SM, Gaur AB, Lengyel E, Peter ME. The miR-200 family determines the epithelial phenotype of cancer cells by targeting the E-cadherin repressors ZEB1 and ZEB2. Genes Dev. 2008;22:894–907. pmid:18381893
  75. 75. Gibbons DL, Lin W, Creighton CJ, Rizvi ZH, Gregory PA, Goodall GJ, et al. Contextual extracellular cues promote tumor cell EMT and metastasis by regulating miR-200 family expression. Genes Dev. 2009;23:2140–51. pmid:19759262
  76. 76. Perdigão-Henriques R, Petrocca F, Altschuler G, Thomas MP, Le MT, Tan SM, et al. miR-200 promotes the mesenchymal to epithelial transition by suppressing multiple members of the Zeb2 and Snail1 transcriptional repressor complexes. Oncogene. 2016 Jan 14;35(2):158–72. pmid:25798844
  77. 77. Teague EM, Print CG, Hull ML. The role of microRNAs in endometriosis and associated reproductive conditions. Hum Reprod Update. 2010 Mar-Apr;16(2):142–65. pmid:19773286
  78. 78. Pankov R, Yamada KM. Fibronectin at a glance. J Cell Sci. 2002 Oct 15;115(Pt 20):3861–3. pmid:12244123
  79. 79. Musgrove EA, Caldon CE, Barraclough J, Stone A, Sutherland RL. Cyclin D as a therapeutic target in cancer. Nat Rev Cancer. 2011 Jul 7;11(8):558–72. pmid:21734724
  80. 80. Kim JK, Diehl JA. Nuclear cyclin D1: an oncogenic driver in human cancer. J Cell Physiol. 2009 Aug;220(2):292–6. pmid:19415697
  81. 81. Shan J, Zhao W, Gu W. Suppression of cancer cell growth by promoting cyclin D1 degradation. Mol Cell. 2009 Nov 13;36(3):469–76. pmid:19917254
  82. 82. Jiao J, Huang L, Ye F, Shi M, Cheng X, Wang X, et al. Cyclin D1 affects epithelial-mesenchymal transition in epithelial ovarian cancer stem cell-like cells. Onco Targets Ther. 2013 Jun 20;6:667–77. pmid:23836980
  83. 83. Tobin NP, Sims AH, Lundgren KL, Lehn S, Landerg G. Cyclin D1, Id1 and EMT in breast cancer. BMC Cancer. 2011 Sep 28;11:417. pmid:21955753
  84. 84. Su H, Jin X, Shen L, Fang Y, Fei Z, Zhang X, et al. Inhibition of cyclin D1 enhances sensitivity to radiotherapy and reverses epithelial to mesenchymal transition for esophageal cancer cells. Tumour Biol. 2016 Apr;37(4):5355–63. pmid:26561473
  85. 85. Mejlvang J, Kriajevska M, Vandewalle C, Chernova T, Sayan AE, Berx G, et al. Direct repression of cyclin D1 by SIP1 attenuates cell cycle progression in cells undergoing an epithelial mesenchymal transition. Mol Biol Cell. 2007 Nov;18(11):4615–24. pmid:17855508
  86. 86. Graham TR, Zhau HE, Odero-Marah VA, Osunkoya AO, Kimbro KS, Tighiouart M et al. Insulin-like growth factor-I-dependent up-regulation of ZEB1 drives epithelial-to-mesenchymal transition in human prostate cancer cells. Cancer Res. 2008 Apr 1;68(7):2479–88. pmid:18381457
  87. 87. Irie HY, Pearline RV, Grueneberg D, Hsia M, Ravichandran P, Kothari N, et al. Distinct roles of Akt1 and Akt2 in regulating cell migration and epithelial-mesenchymal transition. J Cell Biol. 2005 Dec 19;171(6):1023–34. pmid:16365168
  88. 88. Taliaferro-Smith L, Oberlick E, Liu T, McGlothen T, Alcaide T, Tobin R, et al. FAK activation is required for IGF1R-mediated regulation of EMT, migration, and invasion in mesenchymal triple negative breast cancer cells. Oncotarget. 2015 Mar 10;6(7):4757–72. pmid:25749031
  89. 89. Kim HJ, Litzenburger BC, Cui X, Delgado DA, Grabiner BC, Lin X, et al. Constitutively active type I insulin-like growth factor receptor causes transformation and xenograft growth of immortalized mammary epithelial cells and is accompanied by an epithelial-to-mesenchymal transition mediated by NF-kappaB and snail. Mol Cell Biol. 2007 Apr;27(8):3165–75. pmid:17296734
  90. 90. Zhou J, Wang J, Zeng Y, Zhang X, Hu Q, Zheng J, et al. Implication of Epithelial-Mesenchymal Transition in IGF1R-Induced Resistance to EGFR-TKIs in Advanced Non-Small Cell Lung Cancer. Oncotarget. 2015 Dec 29;6(42):44332–45. pmid:26554308