Oxidative Medicine and Cellular Longevity
Volume 2019 (2019), Article ID 1958941, 19 pages
https://doi.org/10.1155/2019/1958941

Research Article

Exosomes Derived from TIMP2-Modified Human Umbilical Cord Mesenchymal Stem Cells Enhance the Repair Effect in Rat Model with Myocardial Infarction Possibly by the Akt/Sfrp2 Pathway

Jing Ni,¹ Xijun Liu,1,2 Yiheng Yin,² Peiyu Zhang,¹ Ya-Wei Xu,1,2 and Zheng Liu1,2

¹Department of Cardiology, Shanghai Tenth People’s Hospital, Shanghai, China
²Pan-Vascular Research Institute, Heart, Lung, and Blood Center, Tongji University School of Medicine, Shanghai, China

Correspondence should be addressed to Zheng Liu; liuz@tongji.edu.cn

Received 8 January 2019; Accepted 11 March 2019; Published 28 April 2019

Academic Editor: László Virág

Copyright © 2019 Jing Ni et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

Exosomes derived from human umbilical cord mesenchymal stem cells (hucMSCs) are a promising new therapeutic option for myocardial infarction (MI). The tissue matrix metalloproteinase inhibitor 2, also known as TIMP2, is a member of the tissue inhibitor family of metalloproteinases. Since TIMP2-mediated inhibition of matrix metalloproteinases (MMPs) is a key determinant of post-MI remodeling, we analyzed the therapeutic effects of exosomes derived from TIMP2-overexpressing hucMSCs (huc-exoTIMP2) on the MI rat model. The huc-exoTIMP2 significantly improved in vivo cardiac function as measured by echocardiography and promoted angiogenesis in MI injury. It also restricted extracellular matrix (ECM) remodeling, as indicated by the reduced collagen deposition. In addition, huc-exoTIMP2 administration increased the in situ expression of the antiapoptotic Bcl-2 and decreased that of the proapoptotic Bax and pro-caspase-9 in the infracted myocardium. Meanwhile, huc-exoTIMP2 upregulated superoxide dismutase (SOD) as well as glutathione (GSH) and decreased the malondialdehyde (MDA) level in MI models. In vitro huc-exoTIMP2 pretreatment could inhibit H₂O₂-mediated H9C2-cardiomyocyte apoptosis and promote human umbilical vein endothelial cell (HUVEC) proliferation, migration, and tube formation, as well as decrease TGFβ-induced MMP2, MMP9, and α-SMA secretion by cardiac fibroblasts (CFs). Besides that, huc-exoTIMP2 pretreatment also increased the expression of Akt phosphorylation in the infarcted myocardium, which may relate to a high level of secreted frizzled-related protein 2 (Sfrp2) in huc-exoTIMP2, indicating a mechanistic basis of its action. Importantly, Sfrp2 knockdown in huc-exoTIMP2 abrogated the protective effects. Taken together, huc-exoTIMP2 improved cardiac function by alleviating MI-induced oxidative stress and ECM remodeling, partly via the Akt/Sfrp2 pathway.

1. Introduction

Myocardial infarction (MI) results in the loss of cardiomyocytes and adverse remodeling of the extracellular matrix (ECM). The major mechanism underlying cardiomyocyte loss in the infarcted myocardium is oxidative stress [1], due to excessive reactive oxygen species (ROS) production, which impairs cellular functions and viability [2]. Therefore, improving cardiomyocyte survival and inhibiting apoptosis may be crucial for improving the prognosis of ischemic disease. In addition, the cardiac fibroblasts could be activated by myocardial injury triggering adverse ECM remodeling and excessive fibrosis. The ECM primarily composes of the type I and the type III collagen, which are crucial to maintain the normal cardiac structure, myocardial force, and myocardial systolic and diastolic coordination. Despite a plethora of treatments for MI, restoration of the scarred myocardial tissue is limited due to the nonrenewable nature of the myocardial cells [3].

Stem cell-based tissue regeneration is a promising therapeutic alternative for MI [4]. Transplantation of stem cells in the acute phase of MI inhibits apoptosis of cardiomyocytes, promotes neoangiogenesis, and reduces the local inflammatory response [5, 6]. The stem cells usually originate from the bone marrow and the fat autograft, as well as the umbilical cord. The human umbilical cord mesenchymal stem cells (hucMSCs) are highly suitable for the treatment of MI due to their high self-renewal ability, low immunogenicity, and fewer ethical issues regarding procurement [7, 8]. Studies have been increasingly focusing on paracrine actions of stem cells in recent years. Ma et al. found that Akt-modified hucMSCs secrete microparticles with a hydrodynamic radii ranging from 50 to 200 nm, which enhanced angiogenesis after MI injury [9]. Timmers et al. showed that the conditioned medium from human embryonic MSCs had the ability to repair myocardial ischemia-reperfusion injury, and the exosomes released from MSCs were the major regenerative factors [10]. Exosomes are cell-derived vesicles that transport proteins, lipids, DNA, and RNA and are involved in signal transduction, immune responses, antigen presentation, and would healing among other cellular processes [11], indicating their potential in bioactive therapies. In fact, hucMSC-derived exosomes have been shown to exert cardioprotective effects [12, 13].

The matrix metalloproteinases (MMPs), a group of proteolytic enzymes, could degrade the ECM and initiate the process of ventricular remodeling [14]. The tissue matrix metalloproteinase inhibitors (TIMPs) regulate MMP activity and maintain the balance between ECM breakdown and synthesis [15]. TIMP2, a member of the TIMP family, regulates the proteolytic activity of all MMPs and is involved in cell differentiation, growth, migration, angiogenesis, and apoptosis [16, 17]. TIMP2 knockout resulted in constitutive MMP9 activation abundantly and adverse MI remodeling in vivo [18]. Li et al. showed that TIMP2 and TIMP1 were increased by an endogenous miR-17 inhibitor, decreased MMP9 activity and infarct size, and improved cardiac function [19]. In fact, an aberrant MMP/TIMP ratio is the key factor driving ventricular remodeling in various cardiovascular diseases [20]. Valacca et al. demonstrated that TIMP2 binding to membrane-type 1 matrix metalloproteinase- (MT1-) MMP protected tumor cells against starvation-induced apoptosis by the regulation of the ERK1/2 and Akt signaling pathway [21]. The secreted frizzled- (Fz-) related protein 2 (Sfrp2), a downstream target of the PI3K/Akt signal pathway, regulates mesenchymal stem cell (MSC) survival [22]. In a recent study, Mastri et al. found an obvious improvement in cardiac function by injecting failing hamster hearts with the antibody targeted against the antifibrotic regulator Sfrp2 [23]. However, a potential involvement of the Akt/Sfrp2 axis in MI, or cardiac regeneration, is not completely clear.

In the present study, MI injury and H₂O₂ were used to induce cardiomyocyte injury with or without huc-exoTIMP2 administration, respectively, in vivo and in vitro. We confirmed that MI could induce cardiomyocyte apoptosis as well as ECM remodeling and huc-exoTIMP2 partially abolished such effect. In addition, we also found that the Akt/Sfrp2 signal pathway may exert the antiapoptotic action on cardiomyocytes partly by inhibiting oxidative stress.

2. Materials and Methods

2.1. Ethics Statement

All the animal procedures were conducted in agreement with the Guidelines of Shanghai Laboratory Animal Center and the Policies on the Use of Humans and Animals in Research of the Shanghai Tenth People’s Hospital (SYXK: 2014-0026) and confirmed to the principles outlined in the Declaration of Helsinki. The experimental animals were treated humanely, and all efforts were made to ease their discomfort.

2.2. Culture and Identification of hucMSCs

The hucMSCs were purchased from Shycbio (Shanghai, China) and seeded into Dulbecco’s modified Eagle’s medium F12 (DMEM/F12) medium containing 10% fetal bovine serum (FBS) and 1% PS (all from Gibco, Thermo Fisher Scientific, Waltham, MA, US) at 37°C with 5% CO₂. The culture medium was changed every 72 hrs. When the adherent reached 80% confluency, they were harvested and treated with 0.05% trypsin/0.5 mM EDTA (Sigma-Aldrich, St. Louis, MO, US), washed with flow cytometry buffer (PBS containing 0.5% FBS and 0.02% sodium azide), and divided into aliquots of 0.5- cells. The cells were cultured with various fluorescein isothiocyanate- (FITC-) conjugated or phycoerythrin- (PE-) conjugated monoclonal antibodies (Santa Cruz Biotechnology, Dallas, TX, US), including CD90, CD73, CD105 and CD45, and for 30 min at 37°C. The labeled cells were detected by a FACScan flow cytometer (Becton Dickinson, Franklin Lakes, NJ, US), and nonspecific IgG-labeled cells were used as controls.

2.3. Osteogenic and Adipogenic Differentiation

The hucMSCs from passage 2 (1- cells/per well) were plated on 24-well plates and cultured in DMEM/F12 containing 10% FBS, 0.1 mM dexamethasone, 10 mM β-glycerophosphate, 50 mg/L ascorbic acid, and 4 mg/ml bFGF for osteogenic differentiation (all from Sigma-Aldrich, St. Louis, MO, US). The medium was replaced every 72 hrs, and 3 weeks later, calcium deposition was detected by alizarin red staining.

For adipogenic differentiation, cells of the 2nd passage were seeded in a 24-well plate in DMEM/F12 containing 10% FBS, 1 mM dexamethasone, and 10 mg/ml insulin (all from Sigma-Aldrich). 2 weeks later, Oil Red O staining was used to measure lipid vesicles. The pictures were captured by an Olympus IX51 light microscope (Olympus Canada Inc., Ontario, Canada).

2.4. Transduction of hucMSCs with Lentivirus-TIMP2

hucMSCs were transduced with the lentiviral-TIMP2 () or lentiviral-NC (empty vector, ) using 8 μg/ml polybrene at 37°C in 1.0 ml serum-free medium for 24 hrs (BioLink, Shanghai, China). 48 hrs after infection, the positively transduced cells showed green fluorescence. The expression level of TIMP2 in the transfected hucMSCs (hucMSCsTIMP2) was detected by using qPCR and Western blotting.

2.5. Harvest and Identification of Exosomes from Lentivirus-hucMSCs

Exosomes were purified from TIMP2-transduced hucMSC- (huc-exoTIMP2-) conditioned media by using ultracentrifugation (Beckman Coulter, Brea, CA, US). Briefly, the hucMSCsTIMP2 were cultured till 80% confluency, washed with PBS, and reseeded in DMEM/F12 (HyClone, GE Healthcare, Waukesha, WI, US) including 10% exosome-free FBS (centrifuged at 100,000g for 8 hrs to eliminate preexisting bovine-derived exosomes) and 1% PS. After 24 hrs, the conditioned medium was centrifuged for 10 min at 2,000g to remove cell debris. The huc-exoTIMP2 were purified from the supernatant by ultracentrifugation at 100,000 g for 70 min. All procedures were carried out at 4°C. Exosomes were finally filtered through 0.22 μm Whatman polycarbonate filters (Whatman, Maidstone, UK) and stored at -80°C. hucMSCs with lentivirus-NC were subjected to the same protocol to obtain the huc-exoNC.

The Hitachi H-7650 transmission electron microscope (Hitachi, Tokyo, Japan) was used to observe the exosomal morphology of both huc-exoNC and huc-exoTIMP2 directly. The BCA protein assay kit (Beyotime, Shanghai, China) was used to measure the protein concentration of exosomes and characterized by Western blot with anti-CD9 and anti-CD63 antibodies (all from Abcam, Cambridge, MA, US).

2.6. Cell Isolation and Culture

Neonatal cardiomyocytes were isolated from Sprague Dawley rats (3 days old) by multiple rounds of digestion using 1% collagenase II (Yishen, Shanghai, China) for 60 min. The digested cells were filtered through a 100 μm mesh (Whatman, Maidstone, UK), centrifuged at 1,000 rpm for 10 min, and resuspended in DMEM containing 20% FBS and 1% PS. After a 45 min incubation, the neonatal cardiomyocytes in suspension were aspirated carefully from the adherent fibroblasts, reseeding in a new culture flask and cultured for another 48 hrs. The media were replaced every three days.

H9C2 cells were seeded in high glucose DMEM and supplemented with 10% FBS and 1% PS. Human umbilical cord vein endothelial cells (HUVECs) were cultured in a complete endothelial cell growth medium (ATCC, Manassas, VA, US).

The cells were treated as follows: (i) H₂O₂ (100 μM for 24 hrs), (ii) TGFβ (10 ng/ml for 24 hrs), (iii) huc-exoNC (50 μg/ml for 6 hrs) followed by H₂O₂ for 24 hrs, (iv) huc-exoNC (50 μg/ml for 6 hrs) followed by TGFβ for 24 hrs, (v) huc-exoTIMP2 (50 μg/ml for 6 hrs) followed by H₂O₂ for 24 hrs, and (vi) huc-exoTIMP2 (50 μg/ml for 6 hrs) followed TGFβ for 24 hrs. Untreated controls were also included. Following the different treatments, the medium was replaced with serum-free medium and cells were incubated for another 24 hrs.

2.7. PKH67 Labeling and Fluorescent Microscopy

The exosomes (huc-exoNC or huc-exoTIMP2) were cultured with 1 μg/ml PKH67 dye (Invitrogen, Waltham, MA, US) for 30 min in the dark, washed with PBS, and centrifugated at 100,000g for 1.5 hrs to remove the unbound dye. H9C2 cardiomyocytes and cardiac fibroblasts were cultured with 50 μg/ml PKH67-labeled exosomes for 1 hr, 6 hrs, 12 hrs, and 24 hrs. The cells were washed by PBS and fixed with 4% paraformaldehyde for 10 min. After counterstaining with 1 mg/ml 4,6-diamidino-2-phenylindole (DAPI, Yishen, Shanghai, China) for 5 min, the cells were observed under a Leica DMI6000B fluorescent microscope (Leica Microsystems Ltd., Wetzlar, Germany).

2.8. Cell Viability Assay

The CCK-8 kit (Dojindo Molecular Technologies Inc., Rockville, MD, US) was used to test cell viability. Briefly, cells were seeded in 96-well plates ( cells/per well) in 100 μl DMEM containing 10% FBS overnight. After pretreatment with different concentrations of huc-exoNC or huc-exoTIMP2 (0.1, 1, 10, and 50 μg/ml) for 24 hrs, 10 μl CCK8 solution was added to each well and incubated at 37°C for 1 hr. The absorbance was measured at 450 nm using an enzyme-linked immunosorbent assay plate reader (Bio-Rad Laboratories, Hercules, CA, US).

2.9. In Vivo Myocardial Infarction Model

Male Sprague Dawley rats (6 weeks old, weighting 130-180 g) were procured from the Shanghai Laboratory Animal Center (Shanghai, China) and housed under standard laboratory conditions for 1 week with free access to food and water. The rats were randomized into four groups: (i) the blank control (), (ii) the sham group (MI with PBS, ), (iii) MI with the huc-exoNC transplantation group (), and (iv) MI with the huc-exoTIMP2 transplantation group (). To induce MI, the rats were anesthetized with pentobarbital (60 mg/kg i.p., Shenggong, Shanghai, China) and ventilated using a SCIREQ flexiVent small animal ventilator (SCIREQ, Montreal, Ontario, Canada) to maintain the body temperature at 37°C during the surgery. Anterior thoracotomy was performed to expose the hearts, and the proximal left descending coronary artery was ligated by a 6-0 silk suture. End-expiratory pressure was applied to fully inflate the lungs. After ligation, the PBS, huc-exoNC (50 μg/ml), and huc-exoTIMP2 (50 μg/ml) were injected at three different sites in the peri-infarct zone with a 28-gauge syringe. Ad libitum feeding was resumed after the surgery. Echocardiography was performed after 30 days post-MI. After the last evaluation, the animals were decapitated and the whole hearts were excised and weighed. A portion of the ventricular tissue was preserved at -80°C for molecular analyses, and the remainder was used for histopathology and study of the infarcted area.

2.10. Echocardiography

Echocardiography was performed using a Vevo 770 system (VisualSonics Inc., Toronto, Canada) under anesthesia with inhalation of 1.5% isoflurane-O₂. During the scan, the rats were positioned in a left lateral decubitus form, and left ventricular (LV) M-mode and two-dimensional images were obtained by parasternal short axis view at the papillary muscle level. The parasternal long axis views were obtained and recorded to ensure that visualization of the mitral and aortic valves and the apex was visualized. The transmission frequency was 10 MHz, the depth 2.5 cm, and the frame rate was 225-350 frames per second. The heart rate was recorded as the R-R interval of the electrocardiogram signal. The left ventricular end-systolic dimension (LVESd) and left ventricular end-diastolic volume (LVEDd) were measured from the M-mode tracing. The ejection fraction (EF%) was calculated as , and the shortening fraction (FS%) used the following equation: . All measurements were made by a single observer blinded to the groups of experiments. An average of three consecutive measurements of each variable was used for further analysis.

2.11. Histopathological Examination of Heart Tissues

Isolated hearts were fixed with 4% paraformaldehyde and embedded in paraffin, and serial 4-5 μm sections were prepared. The sections were stained with hematoxylin and eosin (H&E) for morphological analysis and with Masson’s trichrome (MT) to detect the collagen deposition and smooth muscle thickness. The slides were observed under an Olympus IX51 light microscope (Olympus Canada Inc., Ontario, Canada), and stained cells were counted in 3 randomly selected fields by an investigator blinded to the sample.

2.12. Immunofluorescence Assay

The rats were deeply anesthetized and perfused with ice cold PBS/4% paraformaldehyde, following which the hearts were resected and immersed in 30% sucrose. The tissues were cut into 5 μm sections using a freezing microtome. After blocking in 5% BSA for 1 hr, the sections were incubated overnight at 4°C with CD31 and Lycopersicon esculentum lectin antibodies (1 : 50, Abcam, Cambridge, MA, US). The slides were washed with PBS and then incubated with the fluorochrome-labeled goat anti-rabbit IgG conjugated-secondary antibody or goat anti-mouse IgG conjugated-secondary antibody (1 : 1000, Life Technologies, Grand Island, NY, US) for 1 hr at room temperature in the dark.

Cultured cardiac fibroblasts were fixed in 4% paraformaldehyde for 10 min, permeabilized with 0.2% Triton X-100 (Sigma-Aldrich) for 5 min, and blocked with normal goat serum (Boster, Wuhan, China) for 30 min at room temperature. The cells were incubated overnight at 4°C with the anti-α-SMA antibody (1 : 200, Cell Signaling Technology, Danvers, MA, US), followed by a fluorochrome-labeled goat anti-rabbit IgG conjugated-secondary antibody (1 : 1000, Life Technologies) for 1 hr at room temperature. After that, sections were counterstained with 4,6-diamidino-2-phenylindole (DAPI, Boster Biological Technology, Pleasanton, CA, US). Inverted fluorescence microscopy (Leica Microsystems Ltd., Wetzlar, Germany) was used to capture fluorescent images.

2.13. Measurement of Antioxidant Enzymes and Intracellular Reactive Species Generation

The malondialdehyde (MDA) content, superoxide dismutase (SOD) activity, and glutathione (GSH) concentration were measured in rat heart tissues using assay kits purchased from Jiancheng Bioengineering Institute (Nanjing, China) following the manufacturer’s instructions [24].

To measure the oxidative level, flow cytometry was used to monitor the intracellular ROS. In brief, the cells were seeded on 96-well plates, collected, and incubated with 2,7-dichlorofluorescein-diacetate (DCFH-DA, 1 μM) dye in the dark for 30 min at 37°C. Then, the cells were washed with PBS, and the fluorescent intensity of intracellular ROS was detected by the FACSAria III flow cytometer (Becton Dickinson, Franklin Lakes, NJ, US) with the excitation wavelength at 488 nm and emission wavelengths at 525 nm.

2.14. TUNEL Staining

Terminal deoxynucleotidyl transferase- (TdT-) mediated deoxyuridine triphosphate (dUTP) nick end labeling (TUNEL) was performed using an in situ apoptosis detection kit (Beyotime, Jiangsu, China). Briefly, the heart sections were deparaffinized with xylene, rehydrated with ethanol, and rinsed twice in 0.1 M Tris-HCl buffer (pH 7.4) and then twice with PBS. After blocking the sections with 0.3% H₂O₂ for 10 min at room temperature, TdT and dUTP reactions were performed for 1 hr at 37°C. In addition, the TUNEL assay was performed to analyze the cell apoptosis. Briefly, the cells were fixed in 4% paraformaldehyde and permeabilized in 0.03% Triton X-100. Then, the cells were incubated in TUNEL reaction mixture for 1 hr at 37°C. For the negative control, the TdT enzyme was omitted. Nuclei were counterstained with DAPI, and apoptosis was calculated as the number of TUNEL-positive cells in each group and captured with a Leica (Leica Microsystems Ltd., Wetzlar, Germany) fluorescence microscope.

2.15. Flow Cytometric Analysis of Apoptosis

Early apoptotic cells were detected using an annexin V-fluorescein isothiocyanate (FITC)/propidium iodide (PI) detection kit (Becton Dickinson, Franklin Lakes, NJ, US). Briefly, cells ( cells/well) were harvested from each group and added to 500 μl annexin binding buffer. Subsequently, cells were stained with 5 μl annexin V reagent and 10 μl PI in Ca²⁺ enriched binding buffer for 15 min at 37°C in the dark. Then, cells were analyzed by the FACSAria III flow cytometer (Becton Dickinson), and at least cells were acquired per sample.

2.16. Tube Formation Assay

The formation of tube-like structures by the HUVECs was detected in vivo on ECM gel (Sigma-Aldrich). Briefly, the HUVECs were seeded onto ECM-coated (150 μl/well) plates at the density of cells/well and treated with exosomes (50 μg/ml) in the presence/absence of 100 μM H₂O₂ for 12 hrs. The endothelial network formation was observed and captured under an Olympus IX51 microscope. The numbers and length of the tube structures were counted in three randomly selected fields per well using ImageJ software ver. 1.52.

2.17. Wound Healing Assay

HUVECs were seeded in 6-well plates and cultured till 90% confluency. After switching to serum-free media, the monolayer was scratched with a sterile 200 μl pipette tip, and migration of the cells to the “wound” area was monitored at 0 hr and 12 hrs under an inverted microscope (Olympus IX51, Ontario, Canada). Cell migration was analyzed using ImageJ software ver. 1.52. The experiment was conducted in triplicate.

2.18. RNA Extraction and Real-Time Polymerase Chain Reaction (RT-PCR)

Freshly isolated heart tissues were washed with RNase-free water, and total RNA was isolated using TRIzol reagent (Life Technologies) according to the manufacturer’s instructions. PrimeScript™ RT Reagent Kit (Takara Bio Inc., Shiga, Japan) was used to reverse transcribe cDNAs. The PCR was performed in an Applied Biosystems 7500 Real-Time PCR System (Applied Biosystems, Life Technologies) using an SYBR® Premix Ex Taq™ Reagent Kit (Takara). The reaction conditions were set as follows: 95°C for 10 s, 40 cycles of 95°C for 5 s and 60°C for 31 s, one cycle of 95°C for 15 s, 60°C for 30 s, and 95°C for 15 s. The data were normalized to the internal control GAPDH and analyzed using the 2-ΔΔCT method. Primer sequences used for this study were as follows: MMP2: forward, 5-ACGCTGATGGCGAGTACTGCA-3, reverse, 5-CCATGGTAAACAAGGCTTCGTG-3; MMP9: forward, 5-CCTCTGCATGAAGACGACATAA-3, reverse, 5-GGTCAGGTTTAGAGCCACGA-3; TIMP2: forward, 5-TATTGTGCCCTGGGACACG-3, reverse, 5-GTCCATCCAGAGGCACTCATC-3; and GAPDH: forward, 5-AAACTCACTGGCATGGCCTT-3, reverse, 5-TTAGCAGCTTTCTCCAGGCG-3.

2.19. shRNA Transfection

The target sequence for Sfrp2-specific short hairpin RNA (shRNA, Linker, Shanghai, China) was designed as follows: 5-GATCCGGAAGCTCCAAAGGTATGTGAATCAAGAGTTCACATACCTTTGGAGCTTCTTTTTTGG-3. The shRNA-Sfrp2 (sh-Sfrp2) were transfected into the pLKO.1 lentiviral vector. The hucMSCsTIMP2 were seeded into six-well plates and transfected with the lentivirus using polybrene (10 μg/ml, Sigma-Aldrich). After 6 hrs, the lentiviral media was replaced with the completed culture media for another 48 hrs. An empty vector which only expressed green fluorescent protein (GFP) was used as the negative control (sh-NC). Then, cells were harvested at the indicated time points and detected the infection efficiency by RT-PCR.

2.20. Western Blotting

Cells were harvested and lysed in RIPA buffer (Beyotime, Shanghai, China), and the lysates containing 50 μg protein were boiled for 10 min at 100°C. The samples were loaded and separated in 10%-15% SDS-PAGE gel and then transferred onto polyvinylidene fluoride membranes (Millipore, Billerica, MA, US). The blots were blocked with 5% nonfat dry milk in PBST for 1 hr at room temperature and then incubated overnight at 4°C with primary antibodies against MMP2, MMP9, Bcl2, Bax, pro-caspase-9, TIMP2, phosphorylate Akt, or total Akt (1 : 1000, Santa Cruz Biotechnology) and CD9, CD63, α-SMA, or Sfrp2 (1 : 800, Cell Signaling Technology). After washing with PBST, the blots were incubated with horseradish peroxide goat anti-rabbit secondary antibody or horseradish peroxide goat anti-rat secondary antibody (1 : 10000; Yishen, Shanghai, China) for 1 hr at room temperature. GAPDH was also detected as an internal control (1 : 1000, Millipore). Positive bands were visualized by using the enhanced chemiluminescence kit (Amersham, GE Healthcare, Waukesha, WI, US) and quantified by ImageJ software ver. 1.52.

2.21. Statistics

All the experiments were performed in triplicate unless otherwise indicated. All the data are expressed as mean error of mean (SEM) and compared by one-way ANOVA using the GraphPad Prism 6.0 software (GraphPad Software, San Diego, CA, US), followed by the Bonferroni multiple comparison test. values < 0.05 are considered statistically significant.

3. Results

3.1. Characterization of hucMSCs and hucMSC-Derived Exosomes

hucMSCs cultured in vitro showed the characteristic spindle-shaped morphology and were able to differentiate into adipocytes and osteocytes in response to appropriate inducement (Figure 1(a)). To gain further understanding of hucMSCs, the immunophenotype of the hucMSCs from the third passage was positive for CD90, CD73, and CD105 and negative for CD45, indicating an enriched population of hucMSCs (Figure 1(b)).

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Figure 1: Characterization of hucMSCs and hucMSC-derived exosomes. (a) Representative images of spindle-shaped hucMSCs and terminally differentiated adipogenic (Oil Red O-stained) and osteogenic (alizarin A-stained) cells. Scale bar: 50 μm. (b) Flow cytometric plots showing enriched CD90+, CD73+, CD105+, and CD45- hucMSCs. (c) Mass spectrometry results of the TIMP2 level in hucMSC-derived exosomes. (d) Quantification of TIMP2 mRNA and protein expression in TIMP2-transfected hucMSCs. (e) TEM micrographs showing the morphology of hucMSCNC- and hucMSCTIMP2-derived exosomes. Scale bar: 500 nm/200 nm. (f) Immunoblots showing the expression levels of CD9 and CD63 in hucMSCsNC, hucMSCsTIMP2, huc-exoNC, and huc-exoTIMP2. , , and .

Mass spectrometry analysis showed high endogenous levels of the TIMP2 protein in the hucMSCs-exo (Figure 1(c)), and overexpression of the exogenous TIMP2 in hucMSCs was validated by qPCR and Western blotting (Figure 1(d)). TIMP2 mRNA and the protein level were significantly increased in hucMSCsTIMP2 than in hucMSCsNC.

The exosomes were characterized both morphologically and immunophenotypically. As shown in the TEM micrographs in Figure 1(e), numerous multivesicular bodies were present in the cytoplasm of hucMSCsNC and hucMSCsTIMP2, in addition to the secreted membrane-bound, cup-shaped, exosome-like vesicles (40 to 90 nm in diameter). In addition, huc-exoNC and huc-exoTIMP2 expressed the exosomal markers CD9 and CD63 in a higher extent than hucMSCs (Figure 1(f)). Collectively, these results detected that both hucMSCsNC and hucMSCsTIMP2 secrete exosomes and that these exosomes secreted by these cell populations have similar biochemical characterization.

3.2. hucMSC-Derived Exosomes Could Be Internalized by Cardiomyocytes

The internalization of the exosomes by H9C2 cardiomyocytes was tracked by labelling the huc-exoNC and huc-exoTIMP2 with the fluorescent PKH67. As shown in Figure 2(a), both PKH67-labeled exosomes mainly localized in the cytoplasm of H9C2 cardiomyocytes in a time-independent manner.

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Figure 2: Exosome internalization and cell viability in H9C2 cells in vitro. (a) Representative fluorescent images of H9C2 cells incubated with PKH67-labeled huc-exoNC and huc-exoTIMP2 (green) at 1 hr, 6 hrs, 12 hrs, and 24 hrs and quantitation of PKH67-positive cells. Scale bar: 50 μm. (b) A percentage of viable H9C2 cells was cocultured with different concentrations of exosomes (0.1, 1, 10, and 50 μg/ml) for 24 h and then analyzed with the CCK-8 kit. OD540: optical density at 540 nm. and .

In addition, cells cultured with different concentrations of the exosomes (0.1, 1, 10, and 50 μg/ml) showed no changes in viability (Figure 2(b)), indicating that the hucMSC-derived exosomes had no toxic effects on the H9C2 cardiomyocytes.

3.3. huc-exoTIMP2 Alleviated Cardiac Remodeling and Dysfunction In Vivo

To assess the potential cardioprotective effects of the hucMSC-derived exosomes, huc-exoNC and huc-exoTIMP2 were injected directly into the MI rat myocardium. After 30 days, post-MI cardiac function was measured by echocardiography, and EF%, FS%, LVESd, and LVEDd were evaluated. Compared to the placebo (PBS) group, rats injected with huc-exoTIMP2 showed significantly increased LV contractility (EF%) and FS% post-MI. In addition, the D-value of LVESd and LVEDd in the huc-exoTIMP2 group was lower compared to other groups (Figure 3(a)).

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Figure 3: Effect of huc-exoTIMP2 on post-MI cardiac function. (a) EF%, FS%, LVESd, and LVEDd values at 30 days after injection of exosomes. (b) Representative pictures showing the macroscopic appearance of hearts at 30 days post-MI. Arrows indicate infarcted areas. (c) Heart weight/body weight (HW/BW) ratios in different groups. (d) Representative pictures of H&E and Masson trichrome-stained heart sections in different groups. Scale bar: 50 μm. Blank: rats without surgery; MI+PBS: MI rats treated with PBS; NC: MI rats treated with huc-exoNC; TIMP2: MI rats treated with huc-exoTIMP2. , , and .

Histologically, the infarct size in the huc-exoTIMP2 transplanted rats was significantly reduced compared to the huc-exoNC and placebo groups (Figure 3(b)). Furthermore, huc-exoTIMP2 treatment significantly decreased ventricular dilation as measured in terms of heart weight/body weight ratio (Figure 3(c)), less myocardial remodeling and fibrosis as assessed by an H&E stain and Masson’s trichrome stain (Figure 3(d)) compared with other groups. Taken together, huc-exoTIMP2 showed a potent cardioprotective action in infarcted rat hearts by reversing functional decompensation and pathological remodeling, as well as heart failure.

3.4. huc-exoTIMP2 Attenuated Oxidative Stress-Induced Apoptosis in MI Injury

To confirm whether huc-exoTIMP2 was involved in oxidative stress-induced apoptosis, TUNEL staining was used. As shown in Figure 4(a), a significant decrease in TUNEL+ cells was detected in cardiac sections of huc-exoTIMP2 transplanted rats compared with the placebo groups. Besides that, the MDA concentration was significantly increased, and SOD and GSH activities were decreased in MI injury-induced hearts, while huc-exoTIMP2 administration could reverse this trend (Figure 4(b)). These above intracellular antioxidant factors are all involved in counteracting and clearing ROS [25]. To further investigate how huc-exoTIMP2 inhibited myocardium apoptosis, Western blot was used to determine the apoptosis-related protein expression. As shown in Figure 4(c), the Bcl2 level was significantly decreased, while Bax, as well as pro-caspase-9, was increased at 30 days after MI injury. Upregulation of TIMP2 in huc-exo could reverse the MI injury-induced Bcl2 expression and inhibit Bax and pro-caspase-9 levels. Collectively, these results showed that huc-exoTIMP2 plays an important role in inhibiting myocyte apoptosis and promoting the antioxidant defense system that in turn contribute to the cardiac repair process.

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Figure 4: huc-exoTIMP2 ameliorated oxidative stress-induced cardiomyocyte apoptosis. (a) TUNEL⁺ nuclei in cardiac sections. Scale bar: 50 μm. (b) The levels of MDA, SOD, and GSH concentrations in the heart tissues of different groups. (c) Immunoblots showing the expression levels of Bcl2, Bax, and pro-caspase-9 in heart tissues of different groups; comparison of quantified protein levels. Blank: rats without surgery; MI+PBS: MI rats treated with PBS; NC: MI rats treated with huc-exoNC; TIMP2: MI rats treated with huc-exoTIMP2. , , and .

3.5. huc-exoTIMP2 Promoted Angiogenesis Both In Vivo and In Vitro

Angiogenesis is an important factor influencing ischemic myocardial repair. To determine the angiogenic activity in the differentially treated MI rats, their heart tissue sections were probed for CD31 and lectin. Compared to the placebo-treated MI rats, huc-exoTIMP2 treatment significantly increased the in situ expression levels of CD31 (Figure 5(a)) and lectin (Figure 5(b)).

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Figure 5: huc-exoTIMP2 promoted angiogenesis both in vivo and in vitro. (a) Representative images of heart sections showing in situ expression of CD31 and lectin; quantitative comparison of CD31 and lectin fluorescence intensity. CD31: red, lectin: green, DAPI: blue; scale bar: 50 μm. Blank: rats without surgery; MI+PBS: MI rats treated with PBS; NC: MI rats treated with huc-exoNC; TIMP2: MI rats treated with huc-exoTIMP2. (b) Viability of differentially treated HUVECs. OD540: optical density at 540 nm. (c) Representative images of the wound healing assay showing in vitro migration of HUVECs. Scale bar: 50 μm. (d) Representative images of in vitro tube formation by HUVECs; comparison of tube number and length among different groups. Scale bar: 50 μm. Control: untreated; H₂O₂: treated with H₂O₂ alone; NC: treated with huc-exoNC following H₂O₂; TIMP2: treated with huc-exoTIMP2 following H₂O₂. , , and .

In addition, huc-exoTIMP2 accelerated HUVEC proliferation (Figure 5(c)), migration (Figure 5(d)), and the numbers and length of cell tubes formed in vitro (Figure 5(e)) compared to the other treatment groups. Therefore, huc-exoTIMP2 promoted angiogenesis in the injured myocardium by promoting endothelial cell proliferation and migration.

3.6. huc-exoTIMP2 Inhibited Proliferation of CFs and Downregulated MMP2 and MMP9 Expression

The cellular basis of myocardial hypertrophy following ischemic injury is the excessive proliferation of CFs. As shown in Figure 6(a), CFs pretreated with huc-exoTIMP2 showed significantly lower proliferation rates in a time-dependent manner, in accordance with the protein expression and immunofluorescence level of the myofibroblast marker α-SMA which were decreased by huc-exoTIMP2 pretreatment (Figures 6(b) and 6(c)). During chronic heart failure, the MMP family of extracellular proteins secreted by the CFs drive ECM remodeling [26] by breaking down the collagen [27]. Consistent with the results so far, huc-exoTIMP2 significantly downregulated the levels of MMP2 and MMP9 mRNAs (Figure 6(d)) as well as proteins (Figure 6(e)). Taken together, huc-exoTIMP2 alleviated postischemic myocardial remodeling by blocking CF proliferation and secretion.

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Figure 6: huc-exoTIMP2 inhibited cardiac fibroblast proliferation and MMP2/MMP9 production. (a) Cardiac fibroblast proliferation rate measured at 0, 24, 36, and 48 hrs with the CCK8 assay. OD540: optical density at 540 nm. (b) Immunoblots and (c) immunofluorescence showing the expression levels of α-SMA in cardiac fibroblasts and comparison of quantified levels. (d, e) Expression levels of MMP2 and MMP9 mRNAs and proteins in the cardiac fibroblasts across different groups. Control: untreated; TGFβ: treated with TGFβ alone; NC: treated with huc-exoNC following TGFβ; TIMP2: treated with huc-exoTIMP2 following TGFβ. , , and .

3.7. Regulation of Akt Signaling in MI-Induced Myocardial Apoptosis

Previous studies have shown that TIMP2 interacted with MT1-MMP complexes, activated the Akt pathway, and inhibited tumor cell apoptosis [21]. Therefore, we hypothesized that huc-exoTIMP2 protected the myocardium from apoptosis via the Akt pathway as well. As shown in Figure 7(a), huc-exoTIMP2 preconditioning significantly increased the levels of phosphorylated Akt in the injured myocardium. To further validate the mechanistic role of Akt in postischemic apoptosis, we treated cardiomyocytes exposed to H₂O₂, an in vitro model simulating MI injury, with the Akt inhibitor LY294002. H₂O₂ markedly increased the percentage of apoptotic cells to 29%, which was decreased significantly by huc-exoTIMP2 treatment to 16.9%. However, in the presence of the Akt inhibitor, the apoptosis rate was high at 23.3% (Figure 7(b)). Consistent with this, LY294002 pretreatment also increased the levels of Bax and pro-caspase-9 in H9C2 cells (Figure 7(c)). Taken together, huc-exoTIMP2 protects H9C2 cardiomyocytes from H₂O₂-induced apoptosis partly by activating the Akt signaling pathway.

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Figure 7: huc-exoTIMP2 protects the cardiomyocyte against apoptosis induced by MI injury via the Akt pathway. (a) Immunoblots showing the expression level of phosphorylated Akt in the infarcted rat hearts and quantitative comparison of p-Akt levels across different groups. Blank: rats without surgery; MI+PBS: MI rats treated with PBS; NC: MI rats treated with huc-exoNC; TIMP2: MI rats treated with huc-exoTIMP2. (b) Flow cytometry plots showing annexin V/PI-stained cells; comparison of the percentage of apoptotic cells across different groups. (c) Immunoblots showing expression levels of Bax and pro-caspase-9 and comparison of protein expression across different groups. Control: untreated; H₂O₂: treated with H₂O₂ alone; TIMP2: treated with huc-exoTIMP2 following H₂O₂; LY: treated with LY294002 and huc-exoTIMP2 following H₂O₂. , , and .

3.8. Akt Pathway Is Upstream of Sfrp2 in MI Injury-Induced Response

Sfrp2 is an important mediator of the Akt/mTOR pathway during doxorubicin-induced oxidative stress and apoptosis [28]. Transcriptome sequencing showed a significantly higher Sfrp2 expression level in the huc-exoTIMP2 compared to the huc-exoNC (Figure 8(a)). Furthermore, LY294002 blocked the huc-exoTIMP2-mediated increase of Sfrp2 in H9C2 cardiomyocytes (Figure 8(b)), indicating the involvement of the Akt/Sfrp2 axis in the cardioprotective effects of huc-exoTIMP2. To confirm this hypothesis, we knocked down Sfrp2 in hucMSCsTIMP2 (sh-Sfrp2) and extracted exosomes (sh-Sfrp2-exo) from them, while exosomes secreted by shRNA-NC-hucMSCsTIMP2 were used as a negative control (sh-NC-exo). The RT-PCR and fluorescence GFP results confirmed that Sfrp2 was successfully knocked down in the hucMSCsTIMP2 (Figure 8(c)). The Western blot results found a significant increase in the levels of the proapoptotic proteins Bax and pro-caspase-9 and a concomitant decrease in the antiapoptotic protein Bcl2 (Figure 8(d)) in sh-Sfrp2-exo-induced H9C2 cells under H₂O₂ stimulation, in addition to a substantial increase in the percentage of TUNEL+ apoptotic cells (Figure 8(e)). Moreover, we confirmed the effect of sh-Sfrp2-exo on H₂O₂-induced ROS release. DCFH-DA-stained flow cytometry showed that sh-NC-exo reduced the H₂O₂-induced ROS production in H9C2 cells, while sh-Sfrp2-exo remarkably enhanced ROS levels (Figure 8(f)). Taken together, huc-exoTIMP2 inhibited apoptosis in the H9C2 cardiomyocytes partly by upregulating Sfrp2.

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Figure 8: The Akt/Sfrp2 pathway mediates the cardioprotective effects of huc-exoTIMP2. (a) Transcriptome sequencing in huc-exoTIMP2 and huc-exoNC. (b) Immunoblots showing the expression level of Sfrp2 in H9C2 cells; quantitative comparison of the protein levels. Control: untreated; TIMP2: treated with huc-exoTIMP2; LY: treated with LY294002 and huc-exoTIMP2. (c) RT-PCR and GFP-fluorescent images presenting the transfection efficiency of shRNA-Sfrp2 in hucMSCsTIMP2. (d) Immunoblots showing the expression levels of Bcl2, Bax, and pro-caspase-9 in H9C2 cells under H₂O₂ stimulation; quantitative comparison of the protein levels. (e) Representative fluorescent images of TUNEL+ in H9C2 cells with the sh-Sfrp2-exo pretreatment. TUNEL (red) and DAPI (blue). Scale bar: 50 μm. Control: untreated. (f) The quantitative analysis of the ROS level evaluated by flow cytometry using DCFH-DA.sh-NC-exo, treated with sh-NC-exo following H₂O₂, and sh-Sfrp2-exo, treated with sh-Sfrp2-exo following H₂O₂. , , and .

4. Discussion

Stem cell-based therapies have attracted considerable attention in recent years for various degenerative disorders, and encouraging results have been observed in animal studies and clinical trials. However, large-scale clinical application of regenerative therapies is limited due to the low cellular survival rate in the ischemic microenvironment [29], primarily due to the high levels of ROS that can cause oxidative damage and reduce the viability of the transplanted stem cells [30]. A recent study has demonstrated that human amniotic fluid-derived MSC-utilized hypoxic conditioned media have more paracrine factors, VEGF and TGFβ1, and secretes and enhances the proliferation and migration of human dermal fibroblasts in vitro and wound closure in a skin injury model, as compared to normoxic conditioned media [31]. It is well thought that stem cells exert therapeutic effects by releasing extracellular vesicles or trophic factors [32]. Indeed, cell-to-cell interaction is orchestrated by extracellular vesicles, which are involved in cell communication by transferring protein, mRNA, and lipids to target cells.

Exosomes, a kind of extracellular vesicle, are released from and taken up by different cell types [33, 34]. For example, exosomes released from stem cells have been shown to ameliorate ischemia injury [35] and prevent adverse remodeling of the myocardium [36]. In our work, we successfully exploited lentivirus transfection TIMP2-modified hucMSCs and collected their exosomes. We subsequently demonstrated the exosome’s shape and detected the expression of exosomal markers CD9 and CD63. Importantly, our results suggested that TIMP2-modified hucMSC-derived exosomes ameliorate MI injury, reducing myocardial apoptosis and fibrosis, and improve cardiac function by attenuating oxidative stress and ECM remodeling. Mechanistically, we have investigated the antiapoptotic function and anticardiac fibroblast proliferation, further demonstrating that the effects resulted, at least in part, from activating the Akt/Sfrp2 pathway.

Previous works have showed that oxidative stress in the injured myocardium results in cardiomyocyte apoptosis, which persists throughout the cardiac remodeling and significantly influences the outcome of anti-ischemia therapy [37]. Therefore, blocking apoptosis in the cardiomyocytes can also alleviate cardiac dysfunction and inhibit the development of myocardial remodeling [38, 39]. Since the MMP2 inhibitor TIMP2 blocked oxidative stress-induced apoptosis in a mouse model of ischemic stroke [25], and showed high endogenous levels in primary hucMSCs in our work, we hypothesized its cardioprotective effect in MI injury. We therefore isolated exosomes secreted by TIMP2-overexpressing hucMSCs in order to determine their potential therapeutic effects in a rat model of MI.

The antiapoptotic action of huc-exoTIMP2 in the cardiomyocytes was evaluated in terms of the significantly reduced proportion of TUNEL+ cells, as well as decreased the Bax/Bcl2 ratio and pro-caspase-9 levels. The balance between Bax and Bcl2 is responsible for the integrity of the mitochondrial membrane, and any disruption in this balance results in mitochondrial depolarization and the subsequent activation of the apoptotic cascade [40]. In addition, excessive production of ROS overwhelms the endogenous antioxidant defense system, resulting in massive cellular damage through peroxidation of membrane lipids, sulphydryl enzyme inactivation, and DNA breakdown, which triggers apoptotic cell death [41]. We found low antioxidant enzyme activity in the infarcted rat hearts, which was reversed by huc-exoTIMP2 treatment. Thus, TIMP2 restores the endogenous antioxidant defense system in the myocardium following ischemic injury.

ECM remodeling primarily involves increased MMP9 activity and is accompanied by decreased TIMP2 levels. MMP9 results in excessive collagen deposition and fibrosis in the ECM by inducing antiangiogenic factors in the hypertrophied myocardium [42]. TIMP2 is highly expressed in the myocardium and has the dual actions of activating pro-MMP2 and blocking the activation of MMP2, which inhibit angiogenesis and the development of heart failure [43]. Interestingly, excess TIMP2 also inhibits MMP2 expression [44]. In addition, MMP9 lead to collagen deposition and fibrosis by inducing antiangiogenic factors in the hypertrophied myocardium [42]. In the aortic banding mouse model, TIMP2 knockout resulted in very poor left ventricular function and significant myocardial fibrosis [45]. Consistent with these findings, replenishing TIMP2 in the diseased myocardium proved therapeutic by reducing or preventing disease progression [18]. Furthermore, ROS also activate MMP enzymes and inactivate their endogenous inhibitors [46], which disrupt the balance between matrix deposition and degradation, ultimately leading to myocardial remodeling and impaired cardiac function. In line with all the previous studies, our data suggest that huc-exoTIMP2 decrease the levels of both MMP2 and MMP9 and improved heart function following MI injury with FS% increase, which is similar in magnitude to the increase in LVEF%. Recent clinical trials reported that this improvement in FS% translated to enhanced ventricular function, end-systolic elastance, and preload recruitable stroke work [47, 48].

Angiogenesis, which is vital for repairing the ischemic microenvironment, depends on the migration and proliferation of vascular endothelial cells. Zhang et al. showed that hucMSC-derived exosomes accelerated angiogenesis via the Wnt4/b/catenin signaling pathway [49]. Bian et al. reported that vesicles secreted by the human bone marrow mesenchymal stem cells increased angiogenesis in a rat model of MI [50]. In the present study, we demonstrated that huc-exoTIMP2 increased the number of CD31- and lectin-immunoreactive cells in the MI rat myocardium. It also promoted the proliferation, migration, and tube forming ability of HUVECs under H₂O₂ exposure in vitro. These therapeutic effects might be through the delivery of signaling proteins, enzymes, and transcription factors by exosomes, which could regulate the signaling and function in recipient cells. We found that Akt was significantly higher in huc-exoTIMP2 transplanted myocardial tissue compared with huc-exoNC, indicating that the huc-exoTIMP2 might have delivered some factors to the recipient cells and exerted signal communication.

The Akt pathway is activated by ischemic injury and is pivotal for regulating cardiomyocyte survival [51]. Kim et al. reported that TIMP2 stimulated lung adenocarcinoma cell proliferation by activating the PI3K/Akt pathway activation in an MMP-independent manner [52]. Gnecchi et al. found that Akt-overexpressing MSCs reduced infarct size and restored cardiac function in mice hearts after MI; they postulated that Sfrp2 is a key factor in the protective effect [53]. Sfrp2 was first shown as a downstream target of the PI3K/Akt pathway by Gehmert et al. [54]. Alfaro et al. [55] also found that Sfrp2 inactivated the caspase network and promoted MSC survival. Based on these reports, we determined whether activated Akt induced by huc-exoTIMP2 could upregulate Sfrp2 and whether the latter was involved in maintaining the balance of pro- and antiapoptotic factors. We found that huc-exoTIMP2 could upregulate the Sfrp2 level in H9C2 cardiomyocytes, and the expression of the latter was Akt dependent. In addition, Sfrp2 knockdown in huc-exoTIMP2 increased the Bax/Bcl-2 ratio and pro-caspase-9 levels. Taken together, Akt is upstream of Sfrp2 during the oxidative stress-induced response, thus validating the essential prosurvival role of Sfrp2 [56]. However, the underlying molecular mechanisms need further investigation.

5. Conclusion

In conclusion, exosomes derived from TIMP2-modified hucMSCs repaired the ischemic myocardium by inhibiting cardiomyocyte apoptosis and promoting angiogenesis and ECM remodeling, partly by activating the prosurvival Akt/Sfrp2 pathway. This study establishes a new promising therapeutic strategy against MI, which needs further clinical validation.

Data Availability

The data used to support the findings of this study are included within the article.

Conflicts of Interest

The authors report no conflict of interest.

Acknowledgments

This work was supported by the National Natural Science Foundation of China (Grant numbers 81570303 and 81870246).

References

R. Z. Shi and Q. P. Li, “Improving outcome of transplanted mesenchymal stem cells for ischemic heart disease,” Biochemical and Biophysical Research Communications, vol. 376, no. 2, pp. 247–250, 2008.

K. M. Regula and L. A. Kirshenbaum, “Apoptosis of ventricular myocytes: a means to an end,” Journal of Molecular and Cellular Cardiology, vol. 38, no. 1, pp. 3–13, 2005.

R. Bolli, L. Becker, G. Gross, R. Mentzer Jr., D. Balshaw, and D. A. Lathrop, “Myocardial protection at a crossroads: the need for translation into clinical therapy,” Circulation Research, vol. 95, no. 2, pp. 125–134, 2004.

E. Martin-Rendon, S. Brunskill, C. Doree et al., “Stem cell treatment for acute myocardial infarction,” Cochrane Database of Systematic Reviews, no. 4, article Cd006536, 2008.

B. Hynes, A. H. Kumar, J. O'Sullivan et al., “Potent endothelial progenitor cell-conditioned media-related anti-apoptotic, cardiotrophic, and pro-angiogenic effects post-myocardial infarction are mediated by insulin-like growth factor-1,” European Heart Journal, vol. 34, no. 10, pp. 782–789, 2013.

F. van den Akker, J. C. Deddens, P. A. Doevendans, and J. P. Sluijter, “Cardiac stem cell therapy to modulate inflammation upon myocardial infarction,” Biochimica et Biophysica Acta (BBA) - General Subjects, vol. 1830, no. 2, pp. 2449–2458, 2013.

D. Baksh, R. Yao, and R. S. Tuan, “Comparison of proliferative and multilineage differentiation potential of human mesenchymal stem cells derived from umbilical cord and bone marrow,” Stem Cells, vol. 25, no. 6, pp. 1384–1392, 2007.

M. L. Weiss, C. Anderson, S. Medicetty et al., “Immune properties of human umbilical cord Wharton’s jelly-derived cells,” Stem Cells, vol. 26, no. 11, pp. 2865–2874, 2008.

J. Ma, Y. Zhao, L. Sun et al., “Exosomes derived from Akt-modified human umbilical cord mesenchymal stem cells improve cardiac regeneration and promote angiogenesis via activating platelet-derived growth factor D,” Stem Cells Translational Medicine, vol. 6, no. 1, pp. 51–59, 2017.

L. Timmers, S. K. Lim, F. Arslan et al., “Reduction of myocardial infarct size by human mesenchymal stem cell conditioned medium,” Stem Cell Research, vol. 1, no. 2, pp. 129–137, 2007.

C. Thery, M. Ostrowski, and E. Segura, “Membrane vesicles as conveyors of immune responses,” Nature Reviews. Immunology, vol. 9, no. 8, pp. 581–593, 2009.

X. L. Wang, Y. Y. Zhao, L. Sun et al., “Exosomes derived from human umbilical cord mesenchymal stem cells improve myocardial repair via upregulation of Smad7,” International Journal of Molecular Medicine, vol. 41, no. 5, pp. 3063–3072, 2018.

Y. Zhao, X. Sun, W. Cao et al., “Exosomes derived from human umbilical cord mesenchymal stem cells relieve acute myocardial ischemic injury,” Stem Cells International, vol. 2015, Article ID 761643, 12 pages, 2015.

J. D. Raffetto and R. A. Khalil, “Matrix metalloproteinases and their inhibitors in vascular remodeling and vascular disease,” Biochemical Pharmacology, vol. 75, no. 2, pp. 346–359, 2008.

D. Vanhoutte and S. Heymans, “TIMPs and cardiac remodeling: ‘embracing the MMP-independent-side of the family’,” Journal of Molecular and Cellular Cardiology, vol. 48, no. 3, pp. 445–453, 2010.

P. Sapienza, L. di Marzo, V. Borrelli et al., “Metalloproteinases and their inhibitors are markers of plaque instability,” Surgery, vol. 137, no. 3, pp. 355–363, 2005.

L. Schaefer, X. Han, N. Gretz et al., “Tubular gelatinase A (MMP-2) and its tissue inhibitors in polycystic kidney disease in the Han:SPRD rat,” Kidney International, vol. 49, no. 1, pp. 75–81, 1996.

V. Kandalam, R. Basu, T. Abraham et al., “TIMP2 deficiency accelerates adverse post-myocardial infarction remodeling because of enhanced MT1-MMP activity despite lack of MMP2 activation,” Circulation Research, vol. 106, no. 4, pp. 796–808, 2010.

S. H. Li, J. Guo, J. Wu et al., “miR-17 targets tissue inhibitor of metalloproteinase 1 and 2 to modulate cardiac matrix remodeling,” The FASEB Journal, vol. 27, no. 10, pp. 4254–4265, 2013.

L. Moore, D. Fan, R. Basu, V. Kandalam, and Z. Kassiri, “Tissue inhibitor of metalloproteinases (TIMPs) in heart failure,” Heart Failure Reviews, vol. 17, no. 4-5, pp. 693–706, 2012.

C. Valacca, E. Tassone, and P. Mignatti, “TIMP-2 interaction with MT1-MMP activates the AKT pathway and protects tumor cells from apoptosis,” PLoS One, vol. 10, no. 9, article e0136797, 2015.

M. Mirotsou, Z. Zhang, A. Deb et al., “Secreted frizzled related protein 2 (Sfrp 2) is the key Akt-mesenchymal stem cell-released paracrine factor mediating myocardial survival and repair,” Proceedings of the National Academy of Sciences of the United States of America, vol. 104, no. 5, pp. 1643–1648, 2007.

M. Mastri, Z. Shah, K. Hsieh et al., “Secreted frizzled-related protein 2 as a target in antifibrotic therapeutic intervention,” American Journal of Physiology. Cell Physiology, vol. 306, no. 6, pp. C531–C539, 2014.

B. Wei, M. G. You, J. J. Ling et al., “Regulation of antioxidant system, lipids and fatty acid β-oxidation contributes to the cardioprotective effect of sodium tanshinone IIA sulphonate in isoproterenol-induced myocardial infarction in rats,” Atherosclerosis, vol. 230, no. 1, pp. 148–156, 2013.

N. N. Liu, Z. L. Dong, and L. L. Han, “MicroRNA-410 inhibition of the TIMP2-dependent MAPK pathway confers neuroprotection against oxidative stress-induced apoptosis after ischemic stroke in mice,” Brain Research Bulletin, vol. 143, pp. 45–57, 2018.

F. G. Spinale, “Myocardial matrix remodeling and the matrix metalloproteinases: influence on cardiac form and function,” Physiological Reviews, vol. 87, no. 4, pp. 1285–1342, 2007.

C. J. Malemud, “Matrix metalloproteinases (MMPs) in health and disease: an overview,” Frontiers in Bioscience, vol. 11, no. 1, pp. 1696–1701, 2006.

H. Merino and D. K. Singla, “Secreted frizzled-related protein-2 inhibits doxorubicin-induced apoptosis mediated through the Akt-mTOR pathway in soleus muscle,” Oxidative Medicine and Cellular Longevity, vol. 2018, Article ID 6043064, 11 pages, 2018.

K. Huang, S. Hu, and K. Cheng, “A new era of cardiac cell therapy: opportunities and challenges,” Advanced Healthcare Materials, vol. 8, no. 2, article e1801011, 2018.

M. F. Hill and P. K. Singal, “Right and left myocardial antioxidant responses during heart failure subsequent to myocardial infarction,” Circulation, vol. 96, no. 7, pp. 2414–2420, 1997.

E. K. Jun, Q. Zhang, B. S. Yoon et al., “Hypoxic conditioned medium from human amniotic fluid-derived mesenchymal stem cells accelerates skin wound healing through TGF-β/SMAD2 and PI3K/Akt pathways,” International Journal of Molecular Sciences, vol. 15, no. 1, pp. 605–628, 2014.

A. Rustom, R. Saffrich, I. Markovic, P. Walther, and H. H. Gerdes, “Nanotubular highways for intercellular organelle transport,” Science, vol. 303, no. 5660, pp. 1007–1010, 2004.

A. V. Vlassov, S. Magdaleno, R. Setterquist, and R. Conrad, “Exosomes: current knowledge of their composition, biological functions, and diagnostic and therapeutic potentials,” Biochimica et Biophysica Acta (BBA) - General Subjects, vol. 1820, no. 7, pp. 940–948, 2012.

G. Camussi, M. C. Deregibus, S. Bruno, V. Cantaluppi, and L. Biancone, “Exosomes/microvesicles as a mechanism of cell-to-cell communication,” Kidney International, vol. 78, no. 9, pp. 838–848, 2010.

R. C. Lai, F. Arslan, M. M. Lee et al., “Exosome secreted by MSC reduces myocardial ischemia/reperfusion injury,” Stem Cell Research, vol. 4, no. 3, pp. 214–222, 2010.

F. Arslan, R. C. Lai, M. B. Smeets et al., “Mesenchymal stem cell-derived exosomes increase ATP levels, decrease oxidative stress and activate PI3K/Akt pathway to enhance myocardial viability and prevent adverse remodeling after myocardial ischemia/reperfusion injury,” Stem Cell Research, vol. 10, no. 3, pp. 301–312, 2013.

P. P. Wang, Y. J. Zhang, T. Xie, J. Sun, and X. D. Wang, “MiR-223 promotes cardiomyocyte apoptosis by inhibiting Foxo3a expression,” European Review for Medical and Pharmacological Sciences, vol. 22, no. 18, pp. 6119–6126, 2018.

J. Zhu, K. Yao, Q. Wang et al., “Ischemic postconditioning-regulated miR-499 protects the rat heart against ischemia/reperfusion injury by inhibiting apoptosis through PDCD4,” Cellular Physiology and Biochemistry, vol. 39, no. 6, pp. 2364–2380, 2016.

J. Y. Zhang, F. Wu, X. M. Gu et al., “The blockade of transmembrane Cl⁻ flux mitigates I/R-induced heart injury via the inhibition of calpain activity,” Cellular Physiology and Biochemistry, vol. 35, no. 6, pp. 2121–2134, 2015.

Z. Rupniewska and A. Bojarska-Junak, “Apoptosis: mitochondrial membrane permeabilization and the role played by Bcl-2 family proteins,” Postȩpy Higieny i Medycyny Doświadczalnej (Online), vol. 58, pp. 538–547, 2004.

A. Ilhan, M. Iraz, A. Gurel, F. Armutcu, and O. Akyol, “Caffeic acid phenethyl ester exerts a neuroprotective effect on CNS against pentylenetetrazol-induced seizures in mice,” Neurochemical Research, vol. 29, no. 12, pp. 2287–2292, 2004.

Y. Y. Li, A. M. Feldman, Y. Sun, and C. F. McTiernan, “Differential expression of tissue inhibitors of metalloproteinases in the failing human heart,” Circulation, vol. 98, no. 17, pp. 1728–1734, 1998.

R. K. Nuttall, C. L. Sampieri, C. J. Pennington, S. E. Gill, G. A. Schultz, and D. R. Edwards, “Expression analysis of the entire MMP and TIMP gene families during mouse tissue development,” FEBS Letters, vol. 563, no. 1-3, pp. 129–134, 2004.

S. Givvimani, N. Tyagi, U. Sen et al., “MMP-2/TIMP-2/TIMP-4 versus MMP-9/TIMP-3 in transition from compensatory hypertrophy and angiogenesis to decompensatory heart failure,” Archives of Physiology and Biochemistry, vol. 116, no. 2, pp. 63–72, 2010.

V. Kandalam, R. Basu, L. Moore et al., “Lack of tissue inhibitor of metalloproteinases 2 leads to exacerbated left ventricular dysfunction and adverse extracellular matrix remodeling in response to biomechanical stress,” Circulation, vol. 124, no. 19, pp. 2094–2105, 2011.

D. A. Siwik and W. S. Colucci, “Regulation of matrix metalloproteinases by cytokines and reactive oxygen/nitrogen species in the myocardium,” Heart Failure Reviews, vol. 9, no. 1, pp. 43–51, 2004.

R. R. Makkar, R. R. Smith, K. Cheng et al., “Intracoronary cardiosphere-derived cells for heart regeneration after myocardial infarction (CADUCEUS): a prospective, randomised phase 1 trial,” The Lancet, vol. 379, no. 9819, pp. 895–904, 2012.

J. M. Hare, J. E. Fishman, G. Gerstenblith et al., “Comparison of allogeneic vs autologous bone marrow-derived mesenchymal stem cells delivered by transendocardial injection in patients with ischemic cardiomyopathy: the POSEIDON randomized trial,” JAMA, vol. 308, no. 22, pp. 2369–2379, 2012.

B. Zhang, X. Wu, X. Zhang et al., “Human umbilical cord mesenchymal stem cell exosomes enhance angiogenesis through the Wnt4/β-catenin pathway,” Stem Cells Translational Medicine, vol. 4, no. 5, pp. 513–522, 2015.

S. Bian, L. Zhang, L. Duan, X. Wang, Y. Min, and H. Yu, “Extracellular vesicles derived from human bone marrow mesenchymal stem cells promote angiogenesis in a rat myocardial infarction model,” Journal of Molecular Medicine, vol. 92, no. 4, pp. 387–397, 2014.

X. Li, Q. Huang, M. Wang et al., “Compound K inhibits autophagy-mediated apoptosis through activation of the PI3K-Akt signaling pathway thus protecting against ischemia/reperfusion injury,” Cellular Physiology and Biochemistry, vol. 47, no. 6, pp. 2589–2601, 2018.

H. Kim, H. S. Lee, T. H. Kim, J. S. Lee, S. T. Lee, and S. J. Lee, “Growth-stimulatory activity of TIMP-2 is mediated through c-Src activation followed by activation of FAK, PI3-kinase/AKT, and ERK1/2 independent of MMP inhibition in lung adenocarcinoma cells,” Oncotarget, vol. 6, no. 40, pp. 42905–42922, 2015.

M. Gnecchi, H. He, N. Noiseux et al., “Evidence supporting paracrine hypothesis for Akt-modified mesenchymal stem cell-mediated cardiac protection and functional improvement,” The FASEB Journal, vol. 20, no. 6, pp. 661–669, 2006.

S. Gehmert, S. Sadat, Y. H. Song, Y. Yan, and E. Alt, “The anti-apoptotic effect of IGF-1 on tissue resident stem cells is mediated via PI3-kinase dependent secreted frizzled related protein 2 (Sfrp2) release,” Biochemical and Biophysical Research Communications, vol. 371, no. 4, pp. 752–755, 2008.

M. P. Alfaro, A. Vincent, S. Saraswati et al., “sFRP2 suppression of bone morphogenic protein (BMP) and Wnt signaling mediates mesenchymal stem cell (MSC) self-renewal promoting engraftment and myocardial repair,” The Journal of Biological Chemistry, vol. 285, no. 46, pp. 35645–35653, 2010.

M. P. Alfaro, M. Pagni, A. Vincent et al., “The Wnt modulator sFRP2 enhances mesenchymal stem cell engraftment, granulation tissue formation and myocardial repair,” Proceedings of the National Academy of Sciences of the United States of America, vol. 105, no. 47, pp. 18366–18371, 2008.