Skip to main content
Download PDF

Overexpression of miR-1 in the heart attenuates hippocampal synaptic vesicle exocytosis by the posttranscriptional regulation of SNAP-25 through the transportation of exosomes

Cell Communication and Signaling volume 16, Article number: 91 (2018) Cite this article

Abstract

Background

The link between cardiac diseases and cognitive deterioration has been accepted from the concept of “cardiogenic dementia”, which was proposed in the late 1970s. However, the molecular mechanism is unclarified.

Methods

The two animal models used in this study were cardiac-specific overexpression of microRNA-1-2 transgenic (Tg) mice and a myocardial infarction mouse model generated by left coronary artery ligation (LCA). First, we observed the microRNA-1 (miR-1) level and synaptic vesicles (SV) distribution in the hippocampus using in situ hybridization and transmission electron microscopy (TEM) and evaluated the expression of vesicle exocytosis related proteins by western blotting. Second, we used dual luciferase reporter assay as well as antagonist and miRNA-masking techniques to identify the posttranscriptional regulatory effect of miR-1 on the Snap25 gene. Third, FM1–43 staining was performed to investigate the effect of miR-1 on synaptic vesicle exocytosis. Lastly, we used GW4869 to inhibit the biogenesis and secretion of exosomes to determine the transportation effect of exosomes for miR-1 from the heart to the brain.

Results

Compared with the levels in age-matched WT mice, miR-1 levels were increased in both the hearts and hippocampi of Tg mice, accompanied by the redistribution of SVs and the reduction in SV exocytosis-related protein SNAP-25 expression. In vitro studies showed that SNAP-25 protein expression was down- or upregulated by miR-1 overexpression or inhibition, respectively, however, unchanged by miRNA-masking the 3’UTR of the Snap25 gene. SV exocytosis was inhibited by miR-1 overexpression, which could be prevented by co-transfection with an anti-miR-1 oligonucleotide fragment (AMO-1). The knockdown of miR-1 by hippocampal stereotaxic injection of AMO-1 carried by a lentivirus vector (lenti-pre-AMO-1) led to the upregulation of SNAP-25 expression and prevented SV concentration in the synapses in the hippocampi of Tg mice. The application of GW4869 significantly reversed the increased miR-1 level in the blood and hippocampi as well as reduced the SNAP-25 protein levels in the hippocampi of both Tg and LCA mice.

Conclusion

The overexpression of miR-1 in the heart attenuated SV exocytosis in the hippocampus by posttranscriptionally regulating SNAP-25 through the transportation of exosomes. This study contributes to the understanding of the relationship between cardiovascular disease and brain dysfunction.

Background

The primary function of microRNAs (miRNAs) is posttranscriptionally regulating target protein expression by binding to their mRNA recognition sequences [1]. However, with the increasing number of miRNA studies, miRNAs were found to be stable in various body fluids (i.e., serum, plasma, saliva, urine, breast milk, and tears), and showed potential as biomarkers for various diseases [2,3,4,5,6,7,8,9]. More excitingly, miRNAs are also mediate trans-regulation between different cell types after these molecules are secreted into the interstitial space from donor cells and accepted by close recipient cells with functionally targeting capabilities through the actions of various transporters [10,11,12,13]; miRNAs even mediate long-distance metabolic regulation from adipose to the liver [14] and in cancer metastasis [15, 16]. However, whether miRNAs could mediate long-distance heart-brain communication and act as a link between heart disease and brain dysfunction is largely unknown, which would be very interesting.

MicroRNA-1 (miR-1) is a muscle-enriched miRNA that presents a hundred-fold lower level in the brain than in the heart [17, 18]. Interestingly, by bioinformatics analysis, we found that as a muscle-enriched microRNA, 57% of the targets of miR-1 were distributed in the brain and only 5% of the targets were distributed in the heart of adult mice (Fig. 1). Our previous study demonstrated the behavioural abnormalities in a cardiac-specific microRNA-1-2 (miR-1-2) overexpression transgenic (Tg) mouse model, which was associated with the downregulation of BDNF expression in the hippocampus [18]. Furthermore, a very recent study demonstrated that the overexpression of miR-1 in the heart could induce neuronal microtubule damage [19]. These studies revealed the potential of cardiac-originated miRNAs to regulate brain function. Indeed, clarifying the underlying biological significance of heart-brain communication mediated by miRNAs would provide a new insight into association to the prevention of brain dysfunction.

Fig. 1
figure 1

Distribution of miR-1 targets in different tissues. By uploading the 398 target genes onto the David bioinformatics web site, we obtained the tissue distribution of 358 miR-1 targets. All of the miR-1 targets were classified into 3 parts: targets in foetal tissue, targets in mature tissue and targets associated with tumourigenesis. In each part, we analysed the percentage of miR-1 targets in each kind of tissue. For example, in mature tissue, 57% of the targets are distributed in brain tissue and 5% are located in the heart (red arrow)

Full size image

Synaptic pathology is one of the prominent features of Alzheimer’s disease (AD) or vascular dementia (VaD) [20]. Considering the relationship between cardiovascular diseases and dementia [17, 21,22,23,24,25], we hypothesized that the overexpression of miR-1 in the heart might be involved in heart disease-induced abnormal synaptic plasticity. The study will provide evidence to reveal a novel insight into the molecular mechanism of the heart-to-brain connection and disclose a potential communication between cardiac disease and brain disorder.

Methods

Animals

Adult male C57BL/6 mice and cardiac-specific miR-1 overexpression transgenic (Tg) mice (6–7 months) were housed under a controlled temperature of 23 ± 1 °C and humidity of 55 ± 5%. The animals were maintained on a 12 h artificial dark-light cycle (lights on at 07:00 A.M.) with food (regular chow) and water ad libitum. All animal procedures were approved by the ethics committee of Harbin Medical University and carried out in accordance with the European Communities Council Directive of November 24, 1986 (86/609/EEC).

MiR-1 targets and bioinformatic analysis

We acquired mouse miRNA target genes from 7 miRNA target predicting tools, including PicTar, RNAhybrid, DIANA-microT, RNA22, miRBase Targets, miRanda and TargetScan. To improve the reliability of the predicted miRNA regulations, we only extracted the regulations that were predicted by at least two tools. We obtained 398 target genes. Finally, by uploading the 398 target genes onto the David bioinformatics web site, we obtained the tissue distribution of 358 miR-1 targets. After double verification by literature citation, the percentages of the target gene locations were calculated.

Generation of miR-1 transgenic (Tg) mice

MiR-1 Tg mice were generated as previously described [26]. Sexually immature female C57BL/6 mice (4–5 weeks of age) were used to obtain sufficient quantity of eggs (> 250) for microinjection. The Tg mice used in this study were 5th generation or later. Five- and six-month-old mice (5 M and 6 M) were used in this experiment.

In situ hybridization (ISH)

First, 10 μm paraffin sections were prepared from the hippocampi and hearts of mice. After deparaffinization with xylene and ethanol, the sections were washed 3 times with a phosphate buffer solution (PBS) buffer for 5 min each. Then, proteinase K (40 μg/mL) was applied to deproteinate the sections for 20 min at room temperature. Second, after re-fixing in 4% paraformaldehyde(PFA) for 10 min and acetylating in 1.15% triethanolamine and 0.25% acetic anhydride, the sections were prehybridized in hybridization buffer (50% formamide, 5x standard saline citrate (SSC), 0.1% Tween-20, 50 μg/mL heparin, 500 μg/mL yeast tRNA, and 9.2 mM citric acid for adjustment to pH 6) for 2 h at 37 °C. The digoxigenin (DIG)-labelled detection probes mmu-miR-1 (30 nM,: No. 21378–15) and scramble-miR-1 (mis-miR-1, 30 nM, No.99004–15, Exiqon, Vedbaek, Denmark) were added to the slides and hybridized with the tissue overnight at 50 °C in a humidified chamber. The next day, the slides were washed twice with 5× SSC solution (20× SSC, 3 M NaCl, and 0.3 M sodium citrate) for 20 min each, and 3 times with 50% formamide at 37 °C for 20 min each and 5 times with TBS-T sequentially. After blocking for 1 h in blocking solution (2% goat serum, 2 mg/mL BSA, 0.1% Tween-20, and 1× PBS), the sections were incubated with anti-Digoxigenin-AP (1:1000, product No.11093274, Roche, Indianapolis, IN, USA) in blocking solution overnight at 4 °C. Finally, after washing 4 times with TBS containing 0.1% Tween-20, the slides were treated with developer buffer (0.1 M Tris, 0.1 M NaCl, 0.05 M MgCl2, 0.1%Tween, pH 9.5) for 20 min. Colour development was performed with 1-Step™ NBT/BCIP (product No.34042, Thermo Scientific, Rockford, USA). Images were captured using a microscope (AXIO, Zeiss, Germany).

Mouse model of myocardial infarction

The method was described in a previous study [27]. The male C57BL/6 wild-type mice were divided into two groups: the sham group and the myocardial infarction (MI) group. Briefly, the mice were anaesthetized with sodium pentobarbital (40 mg/kg, intraperitoneal) and placed in the supine position with the upper limbs taped to the table. A 1-cm incision was made along the left side of the sternum, and the muscle layers of the chest wall were bluntly dissected to avoid bleeding. The thorax was cut open at the point of the most pronounced cardiac pulsation, the left anterior descending coronary artery was ligated with a 7-0 silk suture and then the chest was closed. Ischaemia was confirmed by an elevated ST segment of the electrocardiogram. Sham-operated control mice underwent the same surgical procedures except that the suture placed under the left coronary artery was not tied. All surgical procedures were performed under sterile conditions. After occlusion for 6 h, 1 d, 15 d and 30 d, hippocampi were collected for next experiments.

Evaluation of ultrastructure morphology by transmission electron microscopy

For transmission electron microscopy detection, the mice were anaesthetized with sodium pentobarbital (100 mg/kg). The hippocampi were removed and immersed in stationary liquid (pH 7.3) containing 3% glutaraldehyde in 0.1 mmol/L sodium phosphate buffer and 0.45 mmol/L Ca2+. The tissue samples were then fixed in 2% osmic acid (OsO4) in PBS with 1.5% potassium ferricyanide. After dehydration with a concentration gradient of alcohol solutions, the tissues were embedded in Epon with propylene oxide as an intermediary solvent. Ultrathin sections were stained with uranyl acetate and lead citrate. The images were examined under a Hitachi H-7650 electron microscope (Hitachi, H-7650, Tokyo, Japan). To analysee vesicular distribution, 20 synapses without organelles near the presynaptic membrane were selected in each group (3 animals). The active zone was identified by a dark thickened presynaptic membrane with a visible synaptic cleft between the pre- and postsynaptic membranes. Both active zone length and the number of synaptic vesicles were measured using Image J software (National Institutes of Health, US). The total number of synaptic vesicles and vesicles located at 0 nm, 0–50 nm and 50–100 nm distances away from the active zone were counted in each selected pre-synapse [28].

Oligonucleotide synthesis

MiR-1 mimics and AMO-1 for rats were synthesized by Shanghai GenePharma Co., Ltd. (Shanghai, China). AMO-1 contains 2’-O-methyl modifications. In addition, scrambled RNA (mis-miR-1) was used as a negative control. Snap25-masking antisense oligodeoxynucleotides (ODNs) were synthesized by Shanghai Sangon Biotech Co., Ltd., China, and these ODNs complemented the position of 408–430 containing the binding sites of miR-1 located at position 413–420 in the 3’ UTR of Snap25. The nucleotides or deoxynucleotides at both ends of the antisense molecules were locked by a methylene bridge connecting the 2’-O and 4’-C atoms. The sequences of these synthesized oligonucleotides are shown in Table 1.

Table 1 The sequences of the synthesized oligonucleotides
Full size table

Construction of lentivirus vectors

To produce a miR-1 antisense inhibitor, two single-stranded DNA oligonucleotides were designed as follows: (1) pre-AMO-1 (“top strand” oligo: tgctg ATACATACTTCTTTACATTCCAGTTTTGGCCACTGACTGACTGGAATGTAGAAGTATGTAT) and its complementary sequence (“bottom strand” oligo: cctgATACATACTTCTACATTCCAGTCAGTCAGTGGCCAAAACTGGAATGTAAAGAAGTATGTATc); (2) pre-mis-AMO-1 as a negative control (“top strand” oligo: tgctgAAATGTACTGCGCGTGGAGACGTTTTGGCCACTGACTGACGTCTCCACGCAGTACATTT) and its complementary sequence (“bottom strand” oligo: cctgAAATGTACTGCGTGGAGACGTCAGTCAGTGGCCAAAACGTCTCCACGCGCAGTACATTTc). Double-stranded oligonucleotides (ds oligos) were generated by annealing the above two strands with the pcDNA™6.2-GW/± EmGFP-miR vector and transforming the ligated construct into competent Escherichia coli, using a BLOCK-iT pol II miR RNAi expression vector and an EmGFP kit from Invitrogen (Shanghai, China). A pre-miRNA expression cassette was transferred to a Gateway® adapted destination vector utilizing Pol II promoters to form a new miRNA expression clone containing attR substrates. The vector was identified by analysing the plasmid sequence (Invitrogen, Shanghai, China). The lenti-pre-AMO-miR-1 vectors used for the experiments (2.0 μL) contained 1.0 × 108 transducing units (TUs)/mL. Virus suspensions were stored at − 80 °C until use and were briefly centrifuged and kept on ice immediately before injection.

Stereotactic injection of lentiviral vectors

The mice were anaesthetized with sodium pentobarbital (40 mg/kg) by intraperitoneal injection and maintained under anaesthesia using 0.5–1.0% isoflurane. The depth of anaesthesia was monitored by detection of reflexes, heart rate and respiratory rate. After anaesthesia, the mice were placed on a stereotaxic frame (RWB Life Science Co. Ltd., China). Injections were administered in the CA1 area of the hippocampus using a 5-μL Hamilton syringe with a 33-gauge tip needle at − 2.2~ 2.5 mm below the surface of the dura. The injection coordinates relative to the bregma were as follows: anteroposterior (AP), − 2.8 mm; mediolateral (ML), ±3.0 mm; and dorsoventral (DV), 2.2–2.5 (Hamilton, Bonaduz, Switzerland). The needle was maintained in place for another 2 min after injection and was then withdrawn very slowly to avoid backflow of the solution. The accuracies of the injection sites were confirmed by stereotaxic injection of Evans blue (Sigma Chemical Co., St. Louis, Missouri, USA) directly into the hippocampus CA1 subfield [18, 29].

Administration of GW4869 into MI and Tg mice

GW4869 (N,N’Bis[4-(4,5-dihydro-1H-imidazol-2-yl) phenyl]-3,3′-p-phenylene-bis-acrylamide dihydrochloride; MW:577.5 g/mol; Cayman Chemical) was first dissolved in the solution of DMSO as the storage solution at a concentration of 8 mg/mL, which was diluted to a concentration of 0.3 mg/mL by 0.9% NaCl before administration. The method of intraperitoneal injection of GW4869 was used in this study, and the single injection dosage was 200 μl at 0.3 mg/mL for each mouse. Equal volumes of 3.75% DMSO diluted with 0.9% NaCl were injected into mice as a control group. The first injection was performed on the day before LCA surgery for myocardial infarction mice and at the age of 6 M for Tg mice. Thereafter, GW4869 administration was performed 1 times per 2 d for 15 d, and the mice were sacrificed 24 h after the final injection for the further experiments.

Blood sampling

Whole blood samples (0.5 mL per mouse) were collected from the hearts of the anaesthetized mice (sodium pentobarbital, 100 mg/kg, i.p.) via direct venous puncture. Blood was collected into a vacuum blood collection tube containing sodium citrate and was then carefully transferred into an RNase-free tube for RNA extraction [5, 17].

Primary culture of neonatal rat hippocampal and cortical neurons (NRNs)

The primary culturing of NRNs was performed according to procedures that have been previously described in detail [30]. Briefly, hippocampal and cortical regions were collected from rat pups at postnatal day 0 (P0) and placed immediately into ice-cold PBS. The samples were then dissected and incubated in the presence of 0.125% trypsin (Gibco, USA) for 15 min in a water bath at 37 °C. After dispersion, cells were plated onto cell culture plates pre-coated with 10 μg/mL poly-D-lysine (Sigma, USA). The cells were maintained in culture media containing neurobasal medium (Gibco, USA) with 2% B27 supplement (Invitrogen, USA) and 10% foetal bovine serum (FBS, HyClone, Logan, UT) at a density of 1~ 3 × 105 cells/cm2. The cultures were incubated in a 37 °C humidified chamber that was maintained at 5% CO2. The cells were fed by exchanging 50% of the culture media twice a week. The neurons were treated with 5 μM cytosine arabinoside (Sigma, USA) after 3 d in culture to inhibit astrocyte proliferation. For all experiments, neurons were used at 7–10 days after plating.

Transfection procedures

A dose of 75 pmol/mL miR-1, mis-miR-1, AMO-1, Snap25-ODN siRNA or diethyl phosphorocyanidate (DEPC) water was transfected into NRNs using X-treme GENE siRNA transfection reagent (Cat.# 04476093001, Roche, USA) according to the manufacturer’s instructions [29]. The cells were collected for total RNA isolation or protein purification at 48 h post-transfection.

Dual luciferase reporter assay

We cloned the full-length of 3’UTR of the Snap25 gene to generate reporter vectors with miRNA binding sites. The full-length 3’UTR of Snap25 was then amplified by PCR and cloned into the psi-CHECK™-2 luciferase expression vector containing Not1-Xho1 sites. HEK293T cells minimally expressing endogenous miR-1 were used in the luciferase assay. These cells were cultured in DMEM with 10% FBS and 100 μg/mL penicillin/streptomycin. In vitro transfection and luciferase assays were conducted using HEK293T cells (plated at 40%~ 50% confluence and 20 μmol/L miR-1, AMO-1, or mis-miR-1 as well as 0.5 μg psi-CHECK™-2-target DNA firefly luciferase vector, 1 μL blank plasmid and Lipofectamine 2000 (Invitrogen) transfection reagent according to the manufacturer’s instructions. After 48 h, the luciferase activity was measured with a dual luciferase reporter assay kit (Cat.#. E1910, Promega) and a luminometer (GloMax™ 20/20, Promega, USA). Nucleotide-substitution mutations in the 3’UTRs of Snap25 were generated by direct oligomer synthesis. The sequences of constructs were verified [26, 29].

TaqMan qRT-PCR

The levels of miR-1 were quantified using a TaqMan® MicroRNA Reverse Transcription Kit (Cat.#4,366,596, Applied Biosystems) and TaqMan® Gene Expression Master Mix (the target sequences included UGGAAUGUAAAGAAGUGUGUAU (Cat.#002064) for rats and UGGAAUGUAAAGAAGUAUGUAU (Cat.#002222) for mice; Applied Biosystems), and U6 (Cat.# 001973, Applied Biosystems) was used as an internal control. The TaqMan qRT–PCR probes and primers for miR-1 were designed by Invitrogen (USA). qRT-PCR was performed with a thermocycler (ABI Prism® 7500 fast, Applied Biosystems, Foster City, CA) for 40 cycles. The threshold cycle (Ct) was defined as the fractional cycle number at which the fluorescence passed the fixed threshold. PCR was performed as follows: (1) 95 °C for 10 min; (2) 95 °C for 15 s, followed by 60 °C for 1 min (repeat (2) for 40 cycles). The results were normalized against U6 expression levels using the δ–δ Ct method [26].

Western blot analysis

Total protein samples for western blot analysis were extracted from cultured NRNs or the left ventricle and hippocampi of the mice after they were anaesthetized with sodium pentobarbital (100 mg/kg, i.p.). Mouse death was then confirmed by exsanguination according to a previously described method [31]. Hippocampi for primary cell culture were collected from neonatal Sprague-Dawley (SD) rats after the administration of 20% isoflurane and confirmation of death by cervical dislocation. Anti-SNAP-25 (1:1000, ab5666, Abcam, MA, USA), anti-VAMP-2 (1:10000, 104,211, Synaptic Systems, Gottingen, Germany) and anti-Syntaxin-1A (1:5000, 100,111, Synaptic Systems, Gottingen, Germany), anti-Munc-18 (1:1000, 116,002, Synaptic Systems, Gottingen, Germany), anti-CD63 (1:1000, ab193349, Abcam, MA, USA),were used as primary antibodies. β-actin (1:1000, G8795, Sigma, Saint Louis, MO, USA) was selected as an internal control. The blots were detected with an Odyssey Infrared Imaging System (LI-COR Biosciences, Lincoln, NE, USA). The final results were expressed as fold changes compared with the control values.

Detection of synaptic vesicle exocytosis with FM1–43 dyes

FM1–43 fluorescence dye (T35356, Invitrogen, Oregon, USA) was dissolved in deionized, distilled water to make stock solutions (1 mg /mL) and stored at 2–8 °C. After the NRNs were cultured for 10–14 days in the cover glasses, the cell slides were placed in glass bottom of cell culture dishes (Nest, Cat. NO. 801002, China) and washed twice gently with 0.9% NaCl at 37 °C. First, the NRNs were incubated with an FM1–43 fluorescence working solution(10 μg/mL) dissolved in 0.9% NaCl for 3 min at room temperature to allow FM 1–43 binding to the outer membrane of NRNs. Then, 70 mM KCl dissolved in 0.9% NaCl was added to the FM1–43 loaded NRNs for 3 min at room temperature to internalize FM1–43 dye by endocytosis. Subsequently, the NRNs were washed again to remove the extracellular FM1–43 dye with 0.9% NaCl at 37 °C and then placed on a confocal microscope stage. The FM1–43 loaded NRNs were treated with 70 mM KCl solution to elicit synaptic vesicle exocytosis. The declined FM1–43 fluorescence dye signal due to the activated synaptic vesicle exocytosis was monitored by confocal microscopy (Olympus FV1000, Japan), and fluorescence images were acquired every 500 ms [8, 32].

Statistical analysis

The data are described as the mean ± SEM. FM1–43 staining was performed using factorial ANOVA (split-plot design) after performing Mauchly’s test of sphericity with a P > 0.05. Post hoc analyses of significant main effects were further performed using Fisher’s least significant difference test (PLSD) for multiple comparisons. The independent sample test was calculated using the Levene test for equality of variance. If P > 0.05, then an independent Student’s t-test was used for the comparison between two groups. If P < 0.05, then the Kruskal-Wallis rank sum test was performed. One way ANOVA was performed for the comparison among multivariate groups and post hoc analyses of significant main effect ware further examined using Fisher’s PLSD for multiple comparisons. P < 0.05 was considered statistically significant. SAS 9.1 software (serial number: 989155; Institute Inc. China) was used for all statistical analyses.

Results

Abnormal synaptic vesicle distribution in the hippocampi of cardiac-specific miR-1 overexpression Tg mice

To observe whether the overexpression of miR-1 in the heart could induce synaptic pathological remodelling in the brain, a mouse line for the cardiac-specific overexpression of miR-1-2 driven by the α-myosin heavy chain (α-MHC) promoter was developed as described previously [26]. Similar to the previous study [18], miR-1 expression was significantly increased in both the hearts (Fig. 2a) and hippocampi (Fig. 2b) of the Tg mice compared with that in age-matched wild type (WT) mice, as valuated by in situ hybridization technology.

Fig. 2
figure 2

Abnormal synaptic vesicle distribution and related protein expression in the hippocampi of cardiac-specific miR-1 overexpression Tg mice. a-b Elevation of miR-1 levels in the hearts (a) and hippocampi (b) of Tg mice compared with WT mice by in situ hybridization (ISH) using DIG-lablled mmu-miR-1 probes and scramble-miR-1 (mis-miR-1) probes. The positive signal for mmu-miR-1 probes was stained in blue. c Representative electron micrographs of Tg mice. d Morphometric analysis of the total number of SVs in the synapses of neurons from the hippocampi of Tg and WT mice. PLevene < 0.0001, Kruskal-Wallis rank sum test: P < 0.0001. n = 20 synapses from 3 mice for each group. e Quantitative analysis of the distribution of SVs in WT and Tg nerve terminals. 0 nm shell: PLevene = 0.828, Student’s t test: t = − 0.473, P = 0.639; 50 nm shell: PLevene = 0.017, Kruskal-Wallis rank sum test: P = 0.001; 100 nm shell: PLevene = 0.008, Kruskal-Wallis rank sum test: P < 0.0001. n = 20 synapses from 3 mice for each group. f Active zone length was not different between WT and Tg mice. PLevene = 0.016, Kruskal-Wallis rank sum test: P = 0.844. n = 20 active zones from 3 mice for each group. g Schematic diagram of synaptic vesicle fusion. Under the stimulation of Ca2+, Munc-18 switches and binds to syntaxin-1 and assembles SNARE proteins into SNARE-complexes that promote SV fusion with presynaptic membranes. Synaptobrevin 2: VAMP-2. h Representative immunoblotting images of VAMP-2, SNAP-25, Syntaxin-1A, Munc-18. i Statistical analysis of VAMP-2: PLevene = 0.478, Student’s t test: t = − 0.200, P = 0.845; SNAP-25: PLevene = 0.562, Student’s t test: t = 3.463, P = 0.006; Syntaxin-1A: PLevene = 0.670, Student’s t-test: t = 5.067, P < 0.0001. n = 6; Munc-18: PLevene = 0.706, Student’s t-test: t = − 0.656, P = 0.527. n = 6. *P < 0.05; SV: synaptic vesicle

Full size image

Using transmission electron microscopy (TEM) examination, we found that the total number of synaptic vesicles (SVs) in the whole presynaptic area of the hippocampus was significantly increased (Fig. 2c and d). Interestingly, we found that SVs at 0 nm distances from the active zone were the same in the hippocampi of the mice in the two group but they were increased at 50 and 100 nm distances far from the active zone (Fig. 2c and e). However, no difference was observed in the active zone length between the groups (Fig. 2f). These results suggest a blunted fusion process between synaptic vesicles and presynaptic membranes in the hippocampi of the Tg mice. As displayed in Fig. 2g, SV exocytosis is a complex process that is dependent on the cooperation of multiple proteins including the SNARE complex, which is assembled by SNAP-25 (synaptosomal-associated protein 25), VAMP-2 (vesicle associated membrane protein 2, also known as synaptobrevin-2) and syntaxin-1 (also known as HPC-1), which determines the presynaptic release probability by controlling the fusion kinetics [7, 32]. We hence evaluated the expression of SNARE-complex proteins. We found that the SNAP-25 and syntaxin-1A protein levels were significantly reduced, while, VAMP-2 expression was unchanged (Fig. 2h & i). Furthermore, the protein level of Munc-18, which is considered to play a key role in presynaptic vesicle exocytosis by interacting with the SNARE complex [7], was unchanged in the hippocampi of the Tg mice compared with WT mice, (Fig. 2h & i),

MiR-1 targets the Snap25 gene and attenuates synaptic vesicle exocytosis

We next aimed to clarify whether SNAP-25 and syntaxin-1A are the targets of miR-1. By performing computational analysis of miRNA databases (TargetScan 5.1 and miRanda), we found that there is a putative miR-1 binding site in the 3’UTR of the Snap25 gene at the site between 413 bp and 420 bp (Fig. 3a). However, we did not find the binding site of miR-1 on the Stx1a gene (encoding Syntaxin-1A protein). To experimentally verify this finding, we first cloned the full-length 3’UTR of Snap25 into a luciferase-expressing reporter vector (Fig. 3b) and then evaluated the effects of miR-1 on reporter activity in HEK293T cells. The data showed that the co-transfection of the psiCHECK™-2 vector plasmid with miR-1 consistently resulted in a reduction of luciferase activity compared with that observed in transfection of the plasmid alone (Fig. 3c, Renilla/firefly: 1.42 ± 0.08 in blank vs. 0.45 ± 0.03 in miR-1, P < 0.05). Application of a 2′-O-methyl antisense oligoribonucleotide to miR-1 (AMO-1), a specific inhibitor of miR-1, eliminated the repressive effect of miR-1 on the Renilla fluorescence signal (Fig. 3c, Renilla/firefly: 1.52 ± 0.116 in AMO-1 vs. 0.45 ± 0.03 in miR-1, P < 0.05). However, the negative control of both miR-1 (mis-miR-1) and AMO-1 (mis-AMO-1) failed to influence miR-1 action on the Renilla fluorescence signal (Fig. 3c). Furthermore, mutating the binding sites of the Snap25 gene abolished the effect of miR-1 (Fig. 3d), suggesting that these binding sites contribute to the repressive effects of miR-1.

Fig. 3
figure 3

Snap25 is a potential target of miR-1. a Complementarity between the miR-1 seed sequence (5’end 2 ~ 8 nucleotides) and the 3’UTR of mouse’s Snap25 gene as predicted by a computational and bioinformatics-based approach using the Targetscan 5.1 algorithm. Watson-Crick complementarity is marked by a red colour. b The mechanism of the luciferase assay. The full-length 3’UTR of Snap25 was amplified by PCR and cloned into the psiCHECK™-2-control vector. c-d Luciferase reporter gene assay for interactions between miR-1 and its binding site (c) and the mutated binding site (d) in the 3’UTR of the Snap25 gene in HEK293T cells. HEK293T cells were transfected with psiCHECK™-2 vector, miR-1 mimics, AMO-1, or negative control siRNAs (mis-miR-1 and mis-AMO-1) using Lipofectamine 2000 (Wild type: PLevene = 0.086, one-way ANOVA: F = 122.906, P < 0.0001; 3’UTR mut: PLevene = 0.658, One-way ANOVA: F = 3.382, P = 0.054). *P < 0.05 versus psiCHECK™-2-control vector; #P < 0.05, versus miR-1, n = 3 batches of cells for each group

Full size image

To observe whether miR-1 regulates the expression of SNAP-25, we transfected miR-1 and/or AMO-1 directly into NRNs using the X-treme GENE siRNA transfection reagent. The successful transfection of miR-1 and/or AMO-1 was confirmed by miR-1 levels in NRNs detected by qRT-PCR (Fig. 4a). Based on this condition, by immunoblotting analysis, we found that miR-1 effectively inhibited SNAP-25 protein expression by nearly 30% relative to the level of the control group, whereas the scrambled negative control mis-miR-1 failed to affect the protein level (Fig. 4b). In contrast, AMO-1 rescued the miR-1-mediated downregulation of SNAP-25 (Fig. 4b). As predicted, the overexpression of miR-1 did not regulate syntaxin-1A expression in NRNs after transfection with miR-1 and/or AMO-1 (Fig. 4c). To observe whether miR-1 could influence SV number and distribution in vitro, TEM detection was performed. We observed a significantly increased number of SVs in the active zone of NRNs after the transfection of miR-1 for 48 h, however, co-transfection of AMO-1 with miR-1 blocked the miR-1-mediated aggregation of synaptic vesicles inside the synapses (Fig. 4d). FM1–43 fluorescence dyes are widely used to image vesicle exocytosis and endocytosis [8]. We observed that the FM1–43 fluorescent signal in NRNs transfected with mis-miR-1 gradually decreased after 70 mM KCl stimulation (Fig. 4e). The ratio of F/F0 was reduced to 0.5 at 5 s, and further decreased to 0.4 at 10 s after KCl stimulation (Fig. 4f). The transfection of miR-1 markedly blocked the attenuated FM1–43 fluorescent signal induced by KCl, which was reversed by the co-transfection of AMO-1 (Fig. 4e & f).

Fig. 4
figure 4

MiR-1 inhibited SNAP-25 protein expression and presynaptic vesicle release. a Verification of miR-1 in NRNs after transfection. PLevene = 0.001, One-way ANOVA: F = 41.566, P < 0.0001; Fisher’s PLSD test: Pmis-miR-1: miR-1 < 0.0001, PmiR-1: AMO-1 < 0.0001. n = 3 batches of cells for each group. b Expression of SNAP-25 protein in NRNs was downregulated by miR-1 determined by western blot analysis. PLevene = 0.32, One-way ANOVA: F = 4.667, P = 0.008; Fisher’s PLSD test: Pmis-miR-1: miR-1 = 0.04, PmiR-1: AMO-1 = 0.001. n = 5 batches of cells for each group. c The expression of syntaxin-1A protein in NRNs was not influenced by miR-1. PLevene = 0.151, One-way ANOVA: F = 1.033, P = 0.422. d Morphologic change of the transfected primary cultured neurons. e Representative FM1–43 fluorescent signalling changes in each group after 70 mM KCl stimulation. f Co-transfection of AMO-1 with miR-1 improved the decline in FM1–43 signalling decline (F/F0) in NRNs compared with transfection of miR-1 alone. χ2Mauchly = 1652.465, P < 0.0001; Ftotal (19, 1407) = 48.263, P < 0.0001; Fisher’s PLSD test: Pmis-miR-1: miR-1 < 0.0001, PmiR-1: miR-1 + AMO-1 < 0.0001, Pmis-miR-1: miR-1 + AMO-1 < 0.0001. n = 25 neurons from 3 batches of cells for each group

Full size image

To clarify whether the observed changes in SNAP-25 expression and exocytosis in cultured NRNs are the direct results of miR-1 action on the binding sites of this genes, an miRNA-masking antisense ODN fragment (miR-mask) was designed from the 3’UTR of the Snap25 gene sequence. The miR-mask was named Snap25-ODN, which acts on a specific binding site between 408 ~ 430 bp of this gene and minimally influences the effects of miR-1 on other target genes and other binding sites of this gene [33]. As expected from their principle action, Snap25-ODN, unlike AMO-1, did not affect the miR-1 level in cells co-transfected with miR-1 (Fig. 5a). As predicted, Snap25-ODN inhibited the action of miR-1 on SNAP-25 expression (Fig. 5b), suggesting that miR-1 post-transcriptionally regulated SNAP-25 expression by binding to a site located at 413 ~ 420 bp in the 3’UTR of the Snap25 gene. Furthermore, Snap25-ODN successfully prevented the miR-1 overexpression-induced impairment of vesicle exocytosis (Fig. 5c & d). All these results suggested that miR-1 overexpression triggered impaired synaptic vesicle exocytosis, mainly by reducing the SNAP-25 protein level.

Fig. 5
figure 5

MiR-1 influences vesicle exocytosis by inhibiting the expression of SNAP-25 directly. a MiR-1 levels in NRNs transfected with miR-1 and Snap25-ODN. PLevene = 0.041, one-way ANOVA: F = 17.566, P = 0.001; Fisher’s PLSD test: Pmis-miR-1: miR-1 = 0.01, Pmis-miR-1: Snap25-ODN = 0.001. n = 3 batches of cells for each group. b Derepression of SNAP-25 by Snap25-ODN in NRNs co-transfected with miR-1. PLevene = 0.515, one-way ANOVA: F = 18.101, P = 0.001; Fisher’s PLSD test: Pmis-miR-1: miR-1 = 0.01, Pmis-miR-1: Snap25-ODN < 0.0001. *P < 0.05 versus mis-miR-1-control vector; #P < 0.05, versus miR-1. n = 3 batches of cells for each group. c The FM1–43 dye fluorescence change of NRNs co-transfected with miR-1 and Snap25-ODNs. d Snap25-ODN failed to improve the decline in FM1–43 signalling (F/F0) in NRNs transfected with miR-1 alone. χ2Mauchly = 1935.529, P < 0.0001; Ftotal (19, 1407) = 35.946, P < 0.0001; Fisher’s PLSD test: Pmis-miR-1: miR-1 < 0.0001, PmiR-1: miR-1 + Snap25-ODN < 0.0001, Pmis-miR-1: miR-1 + Snap25-ODN = 0.730. n = 25 neurons from 3 batches of cells for each group

Full size image

Furthermore, to determine whether miR-1 is involved in the declined synaptic vesicle exocytosis in the Tg mice, anti-miR-1 oligonucleotide fragments carried by a lentivirus vector (lenti-pre-AMO-1) were stereotaxically injected directly into the CA1 area of the hippocampus bilaterally in the Tg mice at 5 months. The miR-1 levels in the hippocampi of the Tg mice were successfully inhibited by lenti-pre-AMO-1 after injection for 2 months (Fig. 6a). Similar to observations in the in vitro experiments (Fig. 4b), a reduction in SNAP-25 protein levels was observed in the hippocampi of the Tg mice with lenti-pre-mis-AMO-1 which was effectively prevented by lenti-pre-AMO-1 injection (Fig. 6b). Furthermore, lenti-pre-AMO-1 significantly reversed the increased SV number in the Tg mice (Fig. 6c & d) and attenuated SV redistribution at the presynaptic active zone in the hippocampi of the Tg mice (Fig. 6c & e). In this way, lenti-pre-AMO-1 injection did not affect the active zone length compared with that in the uninjected Tg mice (Fig. 2f). These data indicated that the hippocampal overexpression of miR-1 impaired SV exocytosis in Tg mice was associated with the decreased expression of SNAP-25 protein in the hippocampi.

Fig. 6
figure 6

Stereotaxic injection of lenti-pre-AMO-1 into the hippocampi of Tg mice improved SV distribution. a Stereotaxic injection of lenti-pre-AMO-1 into the CA1 domain reduced the miR-1 level in the hippocampi of Tg mice as determined by qRT-PCR analysis. PLevene = 0.01, one-way ANOVA: F = 10.872, P = 0.01; Fisher’s PLSD test: PWT:Tg = 0.005, PTg + lenti-pre-mis-AMO-1::Tg + lenti-pre-AMO-1 = 0.012. n = 3 batches of cells for each group. b Stereotaxic injection of lenti-pre-AMO-1 into the hippocampi of Tg mice derepressed the expression of SNAP-25 protein. PLevene = 0.004, one-way ANOVA: F = 15.700, P < 0.001; Fisher’s PLSD test: PWT:Tg = 0.001, PTg + lenti-pre-mis-AMO-1:Tg + lenti-pre-AMO-1 < 0.0001. n = 6 animals for each group. c Representative electron micrographs showing the effect of stereotaxic injection of lenti-pre-AMO-1 on SVs distribution at presynaptic active zone of Tg mice. d Lenti-pre-AMO-1 prevented an increase in the total number of SVs in the hippocampal synapses of Tg mice. PLevene < 0.003, one-way ANOVA: F = 33.161, P < 0.0001; Fisher’s PLSD test: PWT:Tg < 0.0001, PTg + lenti-pre-mis-AMO-1:Tg + lenti-pre-AMO-1 < 0.0001. n = 20 active zones from 3 mice for each group. e Lenti-pre-AMO-1 redistributed SV location in Tg mice nerve terminals. 0 nm shell: PLevene < 0.012, one-way ANOVA: F = 2.928, P = 0.062; Fisher’s PLSD test: PWT:Tg = 0.596, PTg + lenti-pre-mis-AMO-1: Tg + lenti-pre-AMO-1 = 0.024; 50 nm shell: PLevene = 0.044, one-way ANOVA: F = 7.517, P = 0.01; Fisher’s PLSD test: PWT:Tg = 0.003, PTg + lenti-pre-mis-AMO-1:Tg + lenti-pre-AMO-1 = 0.001; 100 nm shell: PLevene = 0.055, one-way ANOVA: F = 11.161, P < 0.0001; Fisher’s PLSD test: PWT:Tg = 0.014, PTg + lenti-pre-mis-AMO-1:Tg + lenti-pre-AMO-1 < 0.0001. n = 20 synapses s from 3 mice for each group. f Lenti-pre-AMO-1 did not affect the length of active zone. PLevene = 0.551, one-way ANOVA: F = 0.404, P = 0.670; Fisher’s PLSD test: PWT:Tg = 0.940, PTg + lenti-pre-mis-AMO-1:Tg + lenti-pre-AMO-1 = 0.419. n = 20 active zones from 3 mice for each group. *P < 0.05 versus WT; #P < 0.05 versus Tg

Full size image

The cardiac miR-1 overexpression-mediated attenuation of SV exocytosis involves exosomes

We next examined why the overexpression of miR-1 in the heart affects SV exocytosis in the brain. Studies have reported that miRNAs could be secreted into the extracellular space of donor cells and then transported and accepted by recipient cells with functional targeting capabilities [3, 11]. As one kind of miRNA transporter, exosomes not only contain up to 121 miRNAs, including miR-1, miR-15, miR-16, miR-17, miR-18, miR-181, miR-375, lin-4 and let-7 [14], but also show an increase in the serum of the infarcted heart of rats [19, 34]. We hence speculated that exosomes might participate in this process as transporters. To elucidate this issue, we applied GW4869 by intraperitoneal injection to inhibit sphingomyelinase, which was reported to inhibit exosome generation [17]. As illustrated in Fig. 7a, we observed that GW4869 significantly inhibited the reduction in CD63, a marker of exosomes, in Tg mouse hearts, suggesting that the generation of exosomes in the heart was prevented. As predicted, the miR-1 level in the blood (Fig. 7b) and hippocampi (Fig. 7c) of Tg mice were both decreased in Tg mice after GW4869 intraperitoneal injection. Notably, the injection of GW4869 significantly reversed the reduction in SNAP-25 protein in the hippocampi of Tg mice (Fig. 7d).

Fig. 7
figure 7

Inhibition of exosome generation derepressed the expression of SNAP-25 protein in the hippocampi of Tg mice. a Intraperitoneal injection of GW4869 inhibited CD63 expression in the heart of Tg mice at the age of 6 M compared with age-matched Tg mice, as measured by western blotting. PLevene = 0.419, one-way ANOVA: F = 12.778, P = 0.001; Fisher’s PLSD test: PWT:Tg = 0.002, PTg::GW4869 = 0.001. n = 5 animals for each group. b-c Intraperitoneal injection of GW4869 prevented the elevation of miR-1 level in the blood (b: PLevene < 0.001, one-way ANOVA: F = 26.140, P < 0.0001; Fisher’s PLSD test: PWT:Tg < 0.0002, PTg::GW4869 < 0.0001. n = 6 animals for each group) and hippocampi (c: PLevene < 0.001, one-way ANOVA: F = 7.756, P = 0.011; Fisher’s PLSD test: PWT:Tg = 0.004, PTg::GW4869 = 0.0181. n = 4 animals for each group) of Tg mice, as measured by qRT-PCR. d Intraperitoneal injection of GW4869 derepressed SNAP-25 expression in the hippocampi of Tg mice, as measured by western blotting. PLevene = 0.419, one-way ANOVA: F = 12.778, P = 0.001; Fisher’s PLSD test: PWT:Tg = 0.002, PTg::GW4869 = 0.001. n = 6 animals for each group. *P < 0.05 versus WT; #P < 0.05 versus Tg

Full size image

Importantly, miR-1 has been reported to be increased in the blood of both acute myocardial infarction (AMI) rats and patients [5, 35, 36] and hippocampi of myocardial infarction (MI) mice [19]. Could MI also induce impaired presynaptic plasticity and share the same mechanism as that in Tg mice? We first developed an MI animal model by ligating of the left coronary artery (LCA) for 30 days. Similar to the observation in experiments of Tg mice (Figs. 2c & 6c), the number of SVs was significantly increased in MI mice compared with that in sham mice (Fig. 8a & b), and SVs were more concentrated at sites of 50 nm and 100 nm shells from the active zone in MI mice compared with those in age-matched sham mice (Fig. 8a and c). Strikingly, all these changes were prevented by intraperitoneal injection of GW4869 (Fig. 8a-c). However, neither MI nor GW4869 affected the active zone length (Fig. 8d). We then assessed the expression of synaptic fusion-related protein in the hippocampi of MI mice. We found that, consistent with Tg mice, both Munc-18 and VAMP-2 protein levels were unchanged compared with those in the sham control (Fig. 8e). However, SNAP-25 protein expression was significantly reduced from the 15th to the 30th day after LCA (Fig. 8e). Interestingly, although the syntaxin-1A protein level was decreased in the hippocampi of MI mice on the 30th day of LCA, the level was not changed before 15 d (Fig. 8e). Importantly, the intraperitoneal injection of GW4869 into MI mice markedly prevented the increased miR-1 levels (Fig. 8f) and decreased SNAP-25 expression (Fig. 8g) in the hippocampi of MI mice. All these data suggested that the cardiac miR-1 overexpression-mediated attenuation of synaptic vesicle exocytosis involves exosomes.

Fig. 8
figure 8

Inhibition of exosome generation improves MI disrupted SV distribution. a Intraperitoneal injection of GW4869 prevented the synaptic vesicles accumulation at the presynaptic active zone in hippocampal neurons of MI mice. b GW4869 prevented an increase of the total SV number in the synapses in the hippocampi of MI mice. PLevene < 0.0001, one-way ANOVA: F = 19.799, P < 0.0001; Fisher’s PLSD test: Psham: MI < 0.0001, P MI:GW4869 < 0.0001. n = 20 synapses from 3 mice for each group. c GW4869 redistributed SVs at the active zones of synapses in the nerve terminals of Tg mice. 0 nm shell: PLevene = 0.669, one-way ANOVA: F = 3.424, P = 0.039; Fisher’s PLSD test: P sham: MI = 0.360, P MI:GW4869 = 0.012; 50 nm shell: PLevene = 0.016, one-way ANOVA: F = 6.703, P = 0.002; Fisher’s PLSD test: P sham: MI = 0.003, P MI:GW4869 = 0.002; 100 nm shell: PLevene < 0.0001, One way ANOVA: F = 14.785, P < 0.0001; Fisher’s PLSD test: P sham: MI = 0.0001, P MI:GW4869 < 0.0001. n = 20 synapses from 3 mice for each group. d GW4869 did not affect the length of active zone in hippocampi of MI mice. PLevene = 0.271, one-way ANOVA: F = 1.084, P = 0.345; Fisher’s PLSD test: Psham: MI = 0.185, PMI:GW4869 = 0.885. n = 20 active zones from 3 mice for each group. e Expression of SV related proteins in the hippocampi of MI mice. Left: sample bands of immunoblotting images. Right: statistical analysis of Munc 18, VAMP-2, syntaxin- 1A and SNAP-25. *P < 0.05 (f) Intraperitoneal injection of GW4869 prevented the elevation of miR-1 level in the hippocampi of MI mice, as measured by qRT-PCR. PLevene < 0.0001, one-way ANOVA: F = 7.756, P = 0.011; Fisher’s PLSD test: P sham: MI = 0.004, P MI:GW4869 = 0.018. n = 4 animals for each group. g Intraperitoneal injection of GW4869 prevented the decreased SNAP-25 expression in the hippocampi of MI mice, as measured by western blotting. PLevene = 0.265, one-way ANOVA: F = 7.647, P = 0.011; Fisher’s PLSD test: P sham: MI = 0.010, P MI:GW4869 = 0.006. n = 4 animals for each group. *P < 0.05 versus WT; #P < 0.05 versus Tg

Full size image

Discussion

In the present study, we reported that miR-1 overexpression in the heart could result in the attenuation of SV exocytosis, which is controlled by increased miR-1 levels in the hippocampus originating from exosome-mediated transportation from the heart to the brain through circulation. The molecular mechanism involves miR-1 targeting the 3’UTR of the Snap25 gene and post-transcriptionally inhibiting the expression of SNAP-25 protein (Fig. 9). This study improved our understanding of how heart disease induces brain dysfunction at the miRNA level.

Fig. 9
figure 9

Schematic diagrams for the mechanism of the cardiac-specific miR-1 overexpression-induced decline in synaptic vesicle exocytosis. Overexpressed miR-1 in the hearts of Tg and MI mice were secreted into the extracellular space carried by exosomes. Exosomes entered the blood and were transported into the brain through blood circulation. After exosomes enter the brain, they were accepted by neurons and inhibited the expression of SNAP-25 by binding with the target in the 3’UTR of the Snap25 gene. The inhibition of SNAP-25 results in the impairment of vesicle exocytosis through impeding SNARE-complex formation

Full size image

The link between cardiac diseases and cognitive deterioration has been accepted from the concept of “cardiogenic dementia” which was proposed in the late 1970s [37]. However, most studies have focused on cardiac disease-induced chronic brain hypoperfusion (CBH) due to the reduction of cardiac output [22, 24, 38]. Whether heart abnormalities alone could lead to brain damage and even affect cognition is elusive. Using the cardiac-specific overexpression of miR-1-2 in transgenic mice driven by α-MHC, our previous study demonstrated that the overexpression of miR-1 in the hearts of Tg and MI mice could increase its expression in the hippocampus and impaire cognition by post-transcriptionally inhibiting BDNF expression [18, 39]. Because synaptic pathology is a prominent feature of Alzheimer’s disease (AD) or vascular dementia (VaD) [20], we propose that the cardiac overexpression of miR-1 affects synaptic plasticity. Using TEM technique, we observed an increase in miR-1 levels and SV redistribution in the hippocampi of Tg mice, and this phenomenon was reversed by the stereotaxic injection of lenti-pre-AMO-1. This result suggests that the cardiac-specific overexpression of miR-1 could impair synaptic plasticity, which may associate with increased miR-1 levels in the hippocampus. To verify this hypothesis, we performed in vitro experiments and demonstrated that the overexpression of miR-1 led to more synaptic vesicle retention at presynaptic synaptosomes and attenuated KCl-induced FM1–43 fluorescent signal decline, which were prevented by the miR-1 antagonist AMO-1. The decisive step of presynaptic vesicle exocytosis is Ca2+-triggered fusion between synaptic vesicles and presynaptic membranes, which is mediated by the interaction of SNAREs and SM proteins containing SNAP-25, VAMP-2, syntaxin-1A and Munc-18 [7]. Here, we found that both SNAP-25 and syntaxin-1A protein expression levels were decreased. To clarify the molecular mechanism, we used three strategies, including the screening of the bioinformatics database, and in vitro antisense antagonist and miR-masking techniques, and found that miR-1 directly regulates SNAP-25 expression but has no regulatory effect on syntaxin-1A protein expression. Interestingly, a previous study using SNAP-25-deficient neuron reported that the knockdown of SNAP-25 does not modify fusion pore opening or the rate of endocytosis to a degree that could alter Ca2+-triggered release and FM dye release kinetics significantly [40]. In the present study, we observed that miR-1 gain of function could induce a decline in synaptic vesicle exocytosis, which was prevented by shielding the function of SNAP-25 via masking the miR-1 binding site in the 3’UTR of the Snap25 gene located at the site of 413 ~ 420 bp. All these studies implied that miR-1 could induce the impairment of synaptic vesicle exocytosis by inhibiting the expression of SNAP-25 protein. In spite of the fact that SNAP-25 is part of the basic core fusion machinery, the role of SNAP-25 in excitatory- or inhibitory- neurotransmission is controversial [40,41,42,43]. Although we were not able to assess how miR-1 or SNAP-25 affects glutamaterelease or aminobutyric acid neurotransmission, we believe that it is possible that miR-1 or SNAP-25 play a role in both excitatory and inhibitory neurotransmission. However, this hypothesis needs to be studied further. In addition, vesicle release is a cascade response process involving a battery of proteins including synapsins, synaptotagmin-1, Munc-13, Munc-18, compelxins and SNAREs proteins. In this study, we focused on SNARE proteins. Whether the other vesicle-related proteins are also involved in MI- mediated presynaptic plasticity needs to be studied further.

Our previous study demonstrated that the increased miR-1 in the hippocampi of cardiac-specific miR-1-overexpressing Tg mice was not due to endogenous biogenesis, but was associated with exosomes that mediated miR-1 transport from the heart to the brain [18, 19]. Importantly, exosomal miR-1 was increased in both the heart and the blood [34, 44]. Because the physiological process of exosomes as transporters is to release the transported substances into recipient cells by fusing with the recipient cell membrane and then becoming part of the cell membrane, the exosomal miR-1 in the hippocampus might not represent the transported miR-1 level from the heart. In this study, to evaluate the role of cardiac derived exosomes in regulating hippocampal miR-1 levels, we performed an intraperitoneal injection of GW4869 to prevent exosome biogenesis in the heart. We found that GW4869 not only inhibited the expression of CD63 in the heart, a marker of exosomes [17], but also inhibited the increased miR-1 level in both the blood and hippocampi of Tg mice and improved the decreased SNAP-25 expression and SV distribution at the active zone in the hippocampi of Tg mice. In addition, if miR-1 can travel through blood exosomes, then this molecule may reach other brain areas, such as the frontal cortex and even the whole brain, most likely downregulating SNAP-25. This study focused on the hippocampus because the hippocampus is the main brain area associated with spatial memory, especially at the early stage of AD. MI is also considered a risk factor for the onset of AD and may be planned into the preclinical stage of AD. Our previous study demonstrated that miR-1 Tg mice displayed an impairment of spatial memory. However, whether the overexpression of miR-1 in the heart could also induce morphological or functional remodelling in other brain areas and what is the molecular mechanism is very interesting and needs to be clarified further.

Conclusions

Taken together, our findings demonstrate that the overexpression of miR-1 in the heart attenuated synaptic vesicle exocytosis in the hippocampus by posttranscriptionally regulating SNAP-25 through exosome transportation (Fig. 9). This study improved our understanding of the relationship between cardiovascular disease and brain dysfunction at the miRNA levels.

Abbreviations

AMO-1:

anti-miR-1 oligonucleotide fragment

CBH:

chronic brain hypoperfusion

miRNAs:

microRNAs

NRNs:

neonatal rat hippocampal and cortical neurons

ODN:

oligodeoxynucleotides

SNAP-25:

synaptosome-associated protein 25

SNARE:

soluble N-ethylmaleimide-sensitive factor attachment protein receptor

Tg:

transgenic

References

  1. Bartel DP. MicroRNAs: genomics, biogenesis, mechanism, and function. Cell. 2004;116:281–97.

    Article  CAS  Google Scholar 

  2. Gibbings DJ, Ciaudo C, Erhardt M, Voinnet O. Multivesicular bodies associate with components of miRNA effector complexes and modulate miRNA activity. Nat Cell Biol. 2009;11:1143–9.

    Article  CAS  Google Scholar 

  3. Cortez MA, Bueso-Ramos C, Ferdin J, Lopez-Berestein G, Sood AK, Calin GA. MicroRNAs in body fluids--the mix of hormones and biomarkers. Nat Rev Clin Oncol. 2011;8:467–77.

    Article  CAS  Google Scholar 

  4. Chen X, Liang H, Zhang J, Zen K, Zhang CY. Secreted microRNAs: a new form of intercellular communication. Trends Cell Biol. 2012;22:125–32.

    Article  CAS  Google Scholar 

  5. Ai J, Zhang R, Li Y, Pu J, Lu Y, Jiao J, Li K, Yu B, Li Z, Wang R, et al. Circulating microRNA-1 as a potential novel biomarker for acute myocardial infarction. Biochem Biophys Res Commun. 2010;391:73–7.

    Article  CAS  Google Scholar 

  6. Allegra A, Alonci A, Campo S, Penna G, Petrungaro A, Gerace D, Musolino C. Circulating microRNAs: new biomarkers in diagnosis, prognosis and treatment of cancer (review). Int J Oncol. 2012;41:1897–912.

    Article  CAS  Google Scholar 

  7. Sudhof TC. A molecular machine for neurotransmitter release: synaptotagmin and beyond. Nat Med. 2013;19:1227–31.

    Article  Google Scholar 

  8. Gaffield MA, Betz WJ. Imaging synaptic vesicle exocytosis and endocytosis with FM dyes. Nat Protoc. 2006;1:2916–21.

    Article  CAS  Google Scholar 

  9. Vijayan M, Kumar S, Yin X, Zafer D, Chanana V, Cengiz P, Reddy PH. Identification of novel circulatory microRNA signatures linked to patients with ischemic stroke. Hum Mol Genet. 2018;27:2318–29.

    Article  Google Scholar 

  10. Redis RS, Calin S, Yang Y, You MJ, Calin GA. Cell-to-cell miRNA transfer: from body homeostasis to therapy. Pharmacol Ther. 2012;136:169–74.

    Article  CAS  Google Scholar 

  11. Chen X, Liang H, Zhang J, Zen K, Zhang CY. Horizontal transfer of microRNAs: molecular mechanisms and clinical applications. Protein Cell. 2012;3:28–37.

    Article  CAS  Google Scholar 

  12. Zernecke A, Bidzhekov K, Noels H, Shagdarsuren E, Gan L, Denecke B, Hristov M, Koppel T, Jahantigh MN, Lutgens E, et al. Delivery of microRNA-126 by apoptotic bodies induces CXCL12-dependent vascular protection. Sci Signal. 2009;2:ra81.

    Article  Google Scholar 

  13. Vickers KC, Palmisano BT, Shoucri BM, Shamburek RD, Remaley AT. MicroRNAs are transported in plasma and delivered to recipient cells by high-density lipoproteins. Nat Cell Biol. 2011;13:423–33.

    Article  CAS  Google Scholar 

  14. Valadi H, Ekstrom K, Bossios A, Sjostrand M, Lee JJ, Lotvall JO. Exosome-mediated transfer of mRNAs and microRNAs is a novel mechanism of genetic exchange between cells. Nat Cell Biol. 2007;9:654–9.

    Article  CAS  Google Scholar 

  15. Zhang Z, Li X, Sun W, Yue S, Yang J, Li J, Ma B, Wang J, Yang X, Pu M, et al. Loss of exosomal miR-320a from cancer-associated fibroblasts contributes to HCC proliferation and metastasis. Cancer Lett. 2017;397:33–42.

    Article  CAS  Google Scholar 

  16. Casadei L, Calore F, Creighton CJ, Guescini M, Batte K, Iwenofu OH, Zewdu A, Braggio DA, Bill KL, Fadda P, et al. Exosome-derived miR-25-3p and miR-92a-3p stimulate Liposarcoma progression. Cancer Res. 2017;77:3846–56.

    Article  CAS  Google Scholar 

  17. Kosaka N, Iguchi H, Yoshioka Y, Takeshita F, Matsuki Y, Ochiya T. Secretory mechanisms and intercellular transfer of microRNAs in living cells. J Biol Chem. 2010;285:17442–52.

    Article  CAS  Google Scholar 

  18. Ma JC, Duan MJ, Sun LL, Yan ML, Liu T, Wang Q, Liu CD, Wang X, Kang XH, Pei SC, et al. Cardiac over-expression of microRNA-1 induces impairment of cognition in mice. Neuroscience. 2015;299:66–78.

    Article  CAS  Google Scholar 

  19. Sun LL, Duan MJ, Ma JC, Xu L, Mao M, Biddyut D, Wang Q, Yang C, Zhang S, Xu Y, et al. Myocardial infarction-induced hippocampal microtubule damage by cardiac originating microRNA-1 in mice. J Mol Cell Cardiol. 2018;120:12–27.

    Article  CAS  Google Scholar 

  20. Jellinger KA. The pathology of "vascular dementia": a critical update. J Alzheimers Dis. 2008;14:107–23.

    Article  CAS  Google Scholar 

  21. de Toledo Ferraz Alves TC, Ferreira LK, Wajngarten M, Busatto GF. Cardiac disorders as risk factors for Alzheimer's disease. J Alzheimers Dis. 2010;20:749–63.

    Article  Google Scholar 

  22. Monsuez JJ, Gesquiere-Dando A, Rivera S. Cardiovascular prevention of cognitive decline. Cardiol Res Pract. 2011;2011:250970.

    Article  Google Scholar 

  23. Roberts RO, Knopman DS, Geda YE, Cha RH, Roger VL, Petersen RC. Coronary heart disease is associated with non-amnestic mild cognitive impairment. Neurobiol Aging. 2010;31:1894–902.

    Article  Google Scholar 

  24. de la Torre JC. Cardiovascular risk factors promote brain hypoperfusion leading to cognitive decline and dementia. Cardiovasc Psychiatry Neurol. 2012;2012:367516.

    Article  Google Scholar 

  25. Vijayan M, Reddy PH. Stroke, vascular dementia, and Alzheimer's disease: molecular links. J Alzheimers Dis. 2016;54:427–43.

    Article  Google Scholar 

  26. Ai J, Zhang R, Gao X, Niu HF, Wang N, Xu Y, Li Y, Ma N, Sun LH, Pan ZW, et al. Overexpression of microRNA-1 impairs cardiac contractile function by damaging sarcomere assembly. Cardiovasc Res. 2012;95:385-93.

  27. Yang B, Lin H, Xiao J, Lu Y, Luo X, Li B, Zhang Y, Xu C, Bai Y, Wang H, et al. The muscle-specific microRNA miR-1 regulates cardiac arrhythmogenic potential by targeting GJA1 and KCNJ2. Nat Med. 2007;13:486–91.

    Article  CAS  Google Scholar 

  28. Verstegen AM, Tagliatti E, Lignani G, Marte A, Stolero T, Atias M, Corradi A, Valtorta F, Gitler D, Onofri F, et al. Phosphorylation of synapsin I by cyclin-dependent kinase-5 sets the ratio between the resting and recycling pools of synaptic vesicles at hippocampal synapses. J Neurosci. 2014;34:7266–80.

    Article  CAS  Google Scholar 

  29. Ai J, Sun LH, Che H, Zhang R, Zhang TZ, Wu WC, Su XL, Chen X, Yang G, Li K, et al. MicroRNA-195 protects against dementia induced by chronic brain hypoperfusion via its anti-amyloidogenic effect in rats. J Neurosci. 2013;33:3989–4001.

    Article  CAS  Google Scholar 

  30. Chen X, Jiang XM, Zhao LJ, Sun LL, Yan ML, Tian Y, Zhang S, Duan MJ, Zhao HM, Li WR, et al. MicroRNA-195 prevents dendritic degeneration and neuron death in rats following chronic brain hypoperfusion. Cell Death Dis. 2017;8:e2850.

    Article  CAS  Google Scholar 

  31. Che H, Yan Y, Kang XH, Guo F, Yan ML, Liu HL, Hou X, Liu T, Zong DK, Sun LL, et al. MicroRNA-27a promotes inefficient lysosomal clearance in the hippocampi of rats following chronic brain Hypoperfusion. Mol Neurobiol. 2017;54:2595–610.

    Article  CAS  Google Scholar 

  32. Ivannikov MV, Sugimori M, Llinas RR. Synaptic vesicle exocytosis in hippocampal synaptosomes correlates directly with total mitochondrial volume. J Mol Neurosci. 2013;49:223–30.

    Article  CAS  Google Scholar 

  33. Choi WY, Giraldez AJ, Schier AF. Target protectors reveal dampening and balancing of nodal agonist and antagonist by miR-430. Science. 2007;318:271–4.

    Article  CAS  Google Scholar 

  34. Chistiakov DA, Orekhov AN, Bobryshev YV. Cardiac extracellular vesicles in Normal and infarcted heart. Int J Mol Sci. 2016;17:1-18

  35. Cheng Y, Tan N, Yang J, Liu X, Cao X, He P, Dong X, Qin S, Zhang C. A translational study of circulating cell-free microRNA-1 in acute myocardial infarction. Clin Sci (Lond). 2010;119:87–95.

    Article  CAS  Google Scholar 

  36. Liebetrau C, Mollmann H, Dorr O, Szardien S, Troidl C, Willmer M, Voss S, Gaede L, Rixe J, Rolf A, et al. Release kinetics of circulating muscle-enriched microRNAs in patients undergoing transcoronary ablation of septal hypertrophy. J Am Coll Cardiol. 2013;62:992–8.

    Article  CAS  Google Scholar 

  37. Dementia C. Lancet. 1977;1:27–8.

    Google Scholar 

  38. Jefferson AL. Cardiac output as a potential risk factor for abnormal brain aging. J Alzheimers Dis. 2010;20:813–21.

    Article  Google Scholar 

  39. Ma JC, Duan MJ, Li KX, Biddyut D, Zhang S, Yan ML, Yang L, Jin Z, Zhao HM, Huang SY, et al. Knockdown of MicroRNA-1 in the Hippocampus ameliorates myocardial infarction induced impairment of long-term potentiation. Cell Physiol Biochem. 2018;50:1601–16.

    Article  CAS  Google Scholar 

  40. Bronk P, Deak F, Wilson MC, Liu X, Sudhof TC, Kavalali ET. Differential effects of SNAP-25 deletion on Ca2+ −dependent and Ca2+ −independent neurotransmission. J Neurophysiol. 2007;98:794–806.

    Article  CAS  Google Scholar 

  41. Tafoya LC, Mameli M, Miyashita T, Guzowski JF, Valenzuela CF, Wilson MC. Expression and function of SNAP-25 as a universal SNARE component in GABAergic neurons. J Neurosci. 2006;26:7826–38.

    Article  CAS  Google Scholar 

  42. Frassoni C, Inverardi F, Coco S, Ortino B, Grumelli C, Pozzi D, Verderio C, Matteoli M. Analysis of SNAP-25 immunoreactivity in hippocampal inhibitory neurons during development in culture and in situ. Neuroscience. 2005;131:813–23.

    Article  CAS  Google Scholar 

  43. Verderio C, Pozzi D, Pravettoni E, Inverardi F, Schenk U, Coco S, Proux-Gillardeaux V, Galli T, Rossetto O, Frassoni C, Matteoli M. SNAP-25 modulation of calcium dynamics underlies differences in GABAergic and glutamatergic responsiveness to depolarization. Neuron. 2004;41:599–610.

    Article  CAS  Google Scholar 

  44. Cheng Y, Wang X, Yang J, Duan X, Yao Y, Shi X, Chen Z, Fan Z, Liu X, Qin S, et al. A translational study of urine miRNAs in acute myocardial infarction. J Mol Cell Cardiol. 2012;53:668–76.

    Article  CAS  Google Scholar 

Download references

Acknowledgements

The authors would like to thank Pro. Xu Gao for providing the transgenic mice.

Funding

This work was supported by Natural Science Foundation of China (81271207, 81671052 and 81870849 to J. A.).

Availability of data and materials

The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.

Author information

Author notes

  1. Ming-Jing Duan and Mei-Ling Yan contributed equally to this work.

Authors and Affiliations

  1. Department of Pharmacology, College of Pharmacy of Harbin Medical University (the State-Province Key Laboratories of Biomedicine-Pharmaceutics of China), Harbin, 150086, Heilongjiang Province, China

    Ming-Jing Duan, Mei-Ling Yan, Qin Wang, Meng Mao, Dan Su, Lin-Lin Sun, Ke-Xin Li, Yang Qu, Qiang Sun, Xin-Yu Zhang, Si-Yu Huang, Ji-Chao Ma, Tao Ban & Jing Ai

Authors
  1. Ming-Jing Duan
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Mei-Ling Yan
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Qin Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Meng Mao
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Dan Su
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Lin-Lin Sun
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Ke-Xin Li
    View author publications

    You can also search for this author in PubMed Google Scholar

  8. Yang Qu
    View author publications

    You can also search for this author in PubMed Google Scholar

  9. Qiang Sun
    View author publications

    You can also search for this author in PubMed Google Scholar

  10. Xin-Yu Zhang
    View author publications

    You can also search for this author in PubMed Google Scholar

  11. Si-Yu Huang
    View author publications

    You can also search for this author in PubMed Google Scholar

  12. Ji-Chao Ma
    View author publications

    You can also search for this author in PubMed Google Scholar

  13. Tao Ban
    View author publications

    You can also search for this author in PubMed Google Scholar

  14. Jing Ai
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

JA designed, supervised and involved in drafting and editing the manuscript. MJD, MLY, QW, MM, DS, LLS, KXL, YQ, QS, XYZ, SUH, JCM and TB performed the experiments. JA and TB performed statistical analyses. All authors read and approved the final manuscript.

Corresponding authors

Correspondence to Tao Ban or Jing Ai.

Ethics declarations

Consent for publication

Not applicable

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Duan, MJ., Yan, ML., Wang, Q. et al. Overexpression of miR-1 in the heart attenuates hippocampal synaptic vesicle exocytosis by the posttranscriptional regulation of SNAP-25 through the transportation of exosomes. Cell Commun Signal 16, 91 (2018). https://doi.org/10.1186/s12964-018-0303-5

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12964-018-0303-5

Keywords

Cell Communication and Signaling

ISSN: 1478-811X