Research article | Open | Published:
Presenilins regulate synaptic plasticity and mitochondrial calcium homeostasis in the hippocampal mossy fiber pathway
Molecular Neurodegenerationvolume 12, Article number: 48 (2017)
Presenilins play a major role in the pathogenesis of Alzheimer’s disease, in which the hippocampus is particularly vulnerable. Previous studies of Presenilin function in the synapse, however, focused exclusively on the hippocampal Schaffer collateral (SC) pathway. Whether Presenilins play similar or distinct roles in other hippocampal synapses is unknown.
To investigate the role of Presenilins at mossy fiber (MF) synapses we performed field and whole-cell electrophysiological recordings and Ca2+ imaging using acute hippocampal slices of postnatal forebrain-restricted Presenilin conditional double knockout (PS cDKO) and control mice at 2 months of age. We also performed quantitative electron microscopy (EM) analysis to determine whether mitochondrial content is affected at presynaptic MF boutons of PS cDKO mice. We further conducted behavioral analysis to assess spatial learning and memory of PS cDKO and control mice at 2 months in the Morris water maze.
We found that long-term potentiation and short-term plasticity, such as paired-pulse and frequency facilitation, are impaired at MF synapses of PS cDKO mice. Moreover, post-tetanic potentiation (PTP), another form of short-term plasticity, is also impaired at MF synapses of PS cDKO mice. Furthermore, blockade of mitochondrial Ca2+ efflux mimics and occludes the PTP deficits at MF synapses of PS cDKO mice, suggesting that mitochondrial Ca2+ homeostasis is impaired in the absence of PS. Quantitative EM analysis showed normal number and area of mitochondria at presynaptic MF boutons of PS cDKO mice, indicating unchanged mitochondrial content. Ca2+ imaging of dentate gyrus granule neurons further revealed that cytosolic Ca2+ increases induced by tetanic stimulation are reduced in PS cDKO granule neurons in acute hippocampal slices, and that inhibition of mitochondrial Ca2+ release during high frequency stimulation mimics and occludes the Ca2+ defects observed in PS cDKO neurons. Consistent with synaptic plasticity impairment observed at MF and SC synapses in acute PS cDKO hippocampal slices, PS cDKO mice exhibit profound spatial learning and memory deficits in the Morris water maze.
Our findings demonstrate the importance of PS in the regulation of synaptic plasticity and mitochondrial Ca2+ homeostasis in the hippocampal MF pathway.
Alzheimer’s disease (AD) is the most common age-related neurodegenerative disorder characterized by progressive memory loss and cognitive decline. Mutations in the Presenilin genes account for ~90% of all causative mutations in familial AD, highlighting their importance in AD pathogenesis. Genetic studies using conditional gene targeting approaches revealed that Presenilins are essential for learning and memory, synaptic function and age-dependent neuronal survival [1,2,3].
Synaptic dysfunction is widely thought to be one of the earliest key pathogenic events in AD before frank neurodegeneration [1, 4,5,6], and the hippocampal network is particularly vulnerable in AD [7,8,9,10]. The hippocampus consists of three main fields, dentate gyrus (DG), areas CA3 and CA1, and each field displays unique anatomical, molecular, and connectivity patterns [11, 12]. The tri-synaptic circuit conducts synaptic transmission in the hippocampus, and consists of three major excitatory synaptic pathways: perforant path (PP) → DG, mossy fiber (MF) → CA3, and Schaffer collateral (SC) → CA1 . All three hippocampal pathways have been associated with learning and memory [14,15,16], and disruption of the hippocampal network has been implicated in AD. For example, structural and functional MRI analysis of AD patients revealed disruption of the MF-CA3 pathway in patients with mild AD or mild cognitive impairment [17, 18].
We previously reported that inactivation of Presenilins results in impairment of neurotransmitter release, short- and long-term synaptic plasticity at hippocampal SC synapses [1, 2, 19]. However, it was unknown whether Presenilins play similar or distinct roles in the regulation of synaptic function at other hippocampal synapses. In the current study, we focus on the hippocampal MF pathway using the postnatal forebrain-restricted Presenilin conditional double knockout (PS cDKO) mice, in which Presenilins are inactivated in excitatory neurons of the hippocampus beginning at postnatal day 18 [1, 2, 19, 20]. We found that long-term potentiation (LTP), paired-pulse facilitation (PPF) and synaptic facilitation are impaired at MF synapses in PS cDKO mice. Moreover, post-tetanic potentiation (PTP), which lasts longer than facilitation and results from the slow efflux of tetanically accumulated mitochondrial Ca2+ [21, 22], is also reduced at MF synapses in PS cDKO mice. Pharmacological blockade of mitochondrial Ca2+ efflux mimics and occludes PTP deficits at MF synapses of PS cDKO mice, suggesting an impairment of mitochondrial Ca2+ at MF synapses in the absence of Presenilins. However, quantitative electron microscopy (EM) analysis showed similar numbers and areas of mitochondria between control and PS cDKO mice at hippocampal MF presynaptic terminals. Consistent with these findings, Ca2+ imaging of DG granule neurons showed that repeated stimulation-induced cytosolic Ca2+ increases are impaired in granule neurons of PS cDKO mice, and that blockade of mitochondrial Ca2+ release mimics and occludes the Ca2+ homeostasis deficits in PS cDKO granule neurons. Taken together, our study demonstrates the importance of Presenilins in the regulation of synaptic plasticity and mitochondrial Ca2+ homeostasis at hippocampal MF synapses.
The generation and extensive characterization of postnatal forebrain-restricted PS conditional double knockout (PS cDKO) mice were previously reported [1, 2, 19, 20, 23]. Briefly, Northern, in situ hybridization and Western analyses were carried out to confirm the normal PS1 expression in fPS1/fPS1 mice and the inactivation of PS1 in the cerebral cortex of PS cDKO (fPS1/fPS1; PS2 −/− ; αCaMKII-Cre) mice beginning at postnatal day ~18 and complete at ~4 weeks of age [1, 2, 19, 20]. PS cDKO (fPS1/fPS1; PS2 −/− ; αCaMKII-Cre) and control (fPS1/fPS1) mice were in the B6/129 hybrid background. All electrophysiological, Ca2+ imaging, quantitative EM and behavioral analyses were performed in a genotype blind manner using mice at the age of 2 months.
Preparation of brain slices
Hippocampal slices were prepared from both male and female PS cDKO and control mice at 2 months of age. Mice were decapitated after being anesthetized with ketamine (100 mg/kg) + xylazine (10 mg/kg) + acepromazine (3 mg/kg), and the whole brains rapidly removed and placed in ice-cold (4 °C) oxygenated (95% O2/5% CO2) high sucrose and magnesium solution containing (in mM) the following: 200 Sucrose, 25 NaHCO3, 10 Glucose, 3 KCl, 1.25 NaH2PO4, 1.2 Na-pyruvate and 0.4 Na-ascorbate, 7 MgCl2, and 0.5 CaCl2. Horizontal hippocampal slices (400 μm thick) were prepared using a vibratome (VT1200S, Leica, Germany), and transferred to an incubation chamber having oxygenated artificial cerebrospinal fluid (ACSF) containing (in mM) the following: 125 NaCl, 3 KCl, 1.25 NaH2PO4, 1 MgCl2, 2 CaCl2, 25 NaHCO3, 10 Glucose, 1.2 Na-pyruvate and 0.4 Na-ascorbate, adjusted to 310 ± 5 mOsm (pH 7.4). The slices were allowed to recover at 34 °C for 30 min and then placed in a recording chamber constantly perfused with heated ACSF (30 ± 1 °C) and gassed continuously with 95% O2 and 5% CO2. The flow rates of bathing solution and the volume of the recording chamber for slices were 2.2 ml/min and 1.2 ml, respectively. Hippocampal slices were visualized using an upright microscope equipped with differential interference contrast (DIC) optics (BX51WI, Olympus, Japan). The DIC optics was used for visualization of neurons in the course of whole-cell recordings. All experiment procedures were conducted in accordance with guidelines of the Brigham and Women's Hospital Institutional Animal Care and Use Committee and National Institutes of Health.
For extracellular field recordings, stimulation pulses were delivered with a stimulus isolation unit (World Precision Instruments, A365) using a unipolar metal microelectrode. Stimulus electrodes were positioned ~600 μm from the recording electrode in the hilus adjacent to the DG granule cell layer (mossy fibers). Field excitatory postsynaptic potentials (fEPSPs) were recorded in current-clamp mode with ACSF-filled patch pipettes (1.5–2 MΩ). All fEPSPs were recorded with a stimulation strength that yielded 30% of the maximal response. To ensure that MF responses were not contaminated by associational/commissural inputs, the metabotropic glutamate receptor agonist (2S,1′R,2′R,3′R)-2-(2,3-dicarboxycyclopropyl) glycine (DCG IV; 2 μM) was applied at the end of recordings to block MF responses selectively. Data were included only if responses were reduced by more than 80%. All recordings were performed with the GABAA receptor antagonist bicuculline methiodide (10 μM) and NMDA receptor antagonist APV (50 μM) added to the ACSF. Data were collected with a MultiClamp 700B amplifier (Molecular Devices) and digitized at 10 kHz using the A/D converter DIGIDATA 1322A (Molecular Devices). Data were acquired and analyzed using a custom program written with Igor Pro software (Version 6.3; Wave-Metrics) and Clampfit (Version 10.3; Molecular device).
For input/output measurements, 10 traces were averaged for each stimulation intensity, and the amplitude of the fiber volley (FV) was measured relative to the slope of the fEPSP. The stimulation rate was 0.2 Hz. The average linear fit slope was calculated as the slope of the linear input/output relationship for each slice. In LTP recordings, after baseline responses were collected every 15 s for 15 min, LTP was induced by five episodes of theta burst stimulation (TBS) delivered at 0.1 Hz. Each episode contained ten stimulus trains (5 pulses at 100 Hz) delivered at 5 Hz. To generate summary graphs (mean ± SEM), individual experiments were normalized to the baseline, and four consecutive responses were averaged to generate 1 min bins. These were then averaged together to generate the final summary graphs. Paired-pulse facilitation (PPF) was measured as the ratio of the second fEPSP slope relative to the first fEPSP slope, evoked by two identical presynaptic stimuli. Synaptic facilitation was measured as the percentage of the fEPSP slope versus the first fEPSP slope at a given stimulus train in individual slices.
For whole-cell patch clamp experiments, recording pipettes (3–5 MΩ) were filled with a solution containing (in mM) the following: 120 K-gluconate, 10 KCl, 20 HEPES, 4 MgATP, 0.3 NaGTP, 10 phosphocreatine, and 0.1 EGTA with the pH adjusted to 7.30 with KOH (295–300 mOsm). Excitatory postsynaptic currents (EPSCs) at MF synapses were recorded from CA3-pyramidal cells (CA3-PCs) in voltage-clamp mode at a holding potential of −60 mV. The series resistance (Rs) after establishing whole-cell configuration was between 15 and 20 MΩ. Synaptic responses were evoked by extracellular stimulation via a stimulator (Stimulus Isolator A365; WPI) connected to a patch electrode filled with ACSF solution, and placed in stratum lucidum of CA3 field. The stimulus intensity was adjusted such that the baseline EPSC amplitude was in the range between 100 pA and 300 pA. After 10–15 min of stabilization from the break-in, EPSCs were evoked with 0.2 Hz stimulation and recorded for 3–5 min, and followed by high frequency stimulation (HFS: 16 pulses at 100 Hz, delivered 4 times at 0.33 Hz) to induce post-tetanic potentiation (PTP). The PTP was recorded in the presence or absence of CGP37157 (20 μM), inhibitors of mitochondrial Na+/Ca2+ exchanger (NCX), and CGP37157 treatment began 3 min before second HFS and lasted during the PTP recording. The magnitude of PTP was quantified as the average of the first three post-tetanic EPSC amplitudes normalized to the mean baseline amplitudes. EPSC recordings with >20% series resistance change were excluded from data analysis. At the end of each experiment, we examined the effect of DCG IV (2 μM) to confirm that we had studied MF synapses.
For quantitative EM analysis of mitochondria at MF synapses, four PS cDKO and four control mice at the age of 2 months were used. Animals were anaesthetized with sodium pentobarbital and perfused transcardially with physiological saline followed by fixative solution containing 1% glutaraldehyde and 4% paraformaldehyde in 0.1 M phosphate buffer (pH 7.4). Fixed brains were isolated and stored in fixative solution at 4 °C overnight, washed in phosphate buffer, and sectioned coronally on a vibratome (Leica VT 10005) at a thickness of 200 μm. Dorsal hippocampi were carefully excised and post-fixed in 1% OsO4 for 30 min. After rinsing in distilled water and dehydration in an ascending series of ethanol (block-staining with 0.5% uranyl acetate in 70% ethanol) followed by propylene oxide, the hippocampi were embedded in Epon (Fluka) and hardened at 65 °C for two days. Thin sections from stratum lucidum of area CA3 were cut on an ultratome (Leica Ultracut) and mounted on formvar-coated 50-mesh copper grids. Sections were post-stained with lead citrate and subjected to electron microscopy (6200× magnification). The number and area of mitochondria and the area of the presynaptic bouton profiles were quantified. To avoid multiple measurements of the same bouton, randomized sections 5 μm apart from each other were analyzed and at least 10 micrographs per mouse in the cohorts of four animals per condition were used.
Cytosolic Ca2+ ([Ca2+]i) were measured in somata of hippocampal DG granule cells (GCs) using 100 μM Fura-2 pentapotassium salt introduced by a patch pipette. Ca2+ transients were evoked by 10 repetitive depolarizing pulses (2 ms duration from −80 to 0 mV) at various frequencies (1, 5, 10, and 20 Hz) under voltage-clamp conditions. For PTP induction, Ca2+ transients were elicited by 16 repetitive depolarizing pulses at 100 Hz, delivered 4 times at 0.33 Hz. Fluorescence imaging was performed with a 20× water-immersion objective (NA 0.5, UMPlanFln, Olympus), an air-cooling digital monochrome interline CCD camera (ORCA R2, Hamamatsu) and a monochromator (Polychrome V, FEI), which were controlled by a computer and Control Unit for real time TILL Imaging (FEI), running a Live Acqusition Imaging software. Images were taken at 20 Hz with double wavelength excitation at 340 and 380 nm. The ratio r = F 340/F 380 was converted to [Ca2+] values. Calibration parameters were determined using the in vitro calibration method (Invitrogen calibration kit). R min and R max values were calculated as 0.200 and 2.207, respectively.
Mice were housed in a standard 12 h light–dark cycle. Six PS cDKO and six control male mice at 2 months of age were used in the Morris water maze behavioral test. Mice were handled daily for 5 days before training or testing. The Morris water maze is a circular pool 160 cm in diameter. During water maze tasks, mice were trained for 13 days with four trials daily, and the probe tests were administered at days 7 and 13. Mice were released from all four quadrants in a pseudorandom manner during the four training trials. Four visible board cues were hung on the walls during training and probe tests. During the hidden platform training, the platform (10 cm in diameter) was kept submerged under water and maintained in the same position. Each mouse was given four trials daily with a maximum duration of 90 s separated by a minimum of 15 min. If mice did not find the hidden platform, they were guided to the platform and allowed to remain on it for 15 s. The swimming of the mice was monitored using an automated tracking system (HVS Image). After 6 days and 12 days training, two probe tests were performed in the morning of day 7 and day 13 before new training trials. During the probe test at day 7 and day 13, the hidden platform was removed and a 90 s probe test was performed. The mice were released from the opposite position of the platform and searching for the location of the hidden platform according to four visible board cues on the walls. After the 90 s probe test, mice were taken out of the pool and the platform was re-installed in the same position followed by four new training trails.
Statistical analysis was performed using two-tailed Student’s t-test or two-way repeated-measures ANOVA with Bonferroni correction to test for significance for all comparisons of the electrophysiological, quantitative EM analysis, Ca2+ imaging and behavioral results. All data are presented as mean ± SEM.
Impaired long-term potentiation at hippocampal MF synapses in PS cDKO mice
Despite the vulnerability of the hippocampal MF pathway in AD [17, 18], it was unknown whether Presenilins are involved in the regulation of synaptic function at MF synapses. We therefore performed electrophysiological recordings using acute hippocampal slices of forebrain-restricted PS cDKO mice at 2 months of age to investigate whether PS is required for synaptic transmission and plasticity at the MF pathway. We previously reported that Presenilins are inactivated in excitatory neurons of the hippocampus in these PS cDKO mice, beginning at postnatal day 18 and complete at ~1 month of age, and that there is no significant reduction of neurons and synapses in PS cDKO mice at 2 months of age [1,2,3, 19, 20].
We first evaluated basal synaptic transmission by quantifying the initial slope of evoked field excitatory postsynaptic potential (fEPSP) and the amplitude of the fiber volley (FV), which is a measure of the number of recruited axons. Input/output (I/O) curves obtained by plotting the amplitude of FV versus the fEPSP slope in the presence of blockers of NMDA (50 μM APV) and GABAA receptors (10 μM bicuculline) are similar between PS cDKO and control mice, indicating that basal synaptic transmission is normal in the absence of Presenilins (Fig. 1a). We further examined the effects of Presenilins inactivation on LTP at MF synapses. LTP induced by five trains of theta burst stimulation (TBS) is significantly impaired at MF synapses in PS cDKO mice (Fig. 1b). The magnitude of LTP measured during the last 10 min post-induction (50–60 min) is significantly lower in PS cDKO mice (130.9 ± 2.8%), relative to the control (150.5 ± 3.3%; unpaired t-test, p < 0.001). Furthermore, the magnitude of LTP measured during the first 10 min of recording is much lower in PS cDKO mice (136.9 ± 8.7%) relative to controls (189.6 ± 7.9%; unpaired t-test, p < 0.001). To determine whether the responses measured at the MF pathway might be contaminated with associational/commissural inputs, we continued the recording in the presence of the metabotropic glutamate receptor 2 (mGluR2) agonist DCG IV (2 μM), which suppresses transmission at MF synapses . Indeed, LTP at MF synapses was blocked in the presence of DCG IV, confirming that the LTP measured was specific for MF synapses. Together, these results demonstrate that similar to SC synapses, Presenilins are essential for LTP induction at hippocampal MF synapses.
Impaired short-term plasticity at hippocampal MF synapses in PS cDKO mice
Paired-pulse facilitation (PPF) and frequency facilitation are two forms of presynaptic short-term plasticity, which are induced by two closely spaced stimuli or short trains of higher frequency stimulation, respectively. To examine whether loss of PS function affects PPF and frequency facilitation in the hippocampal MF pathway, we recorded fEPSPs at MF synapses onto CA3 pyramidal neurons in PS cDKO mice. We found that PPF is significantly reduced in PS cDKO mice relative to the control, indicating impairment of short-term plasticity at MF synapses of PS cDKO mice (F1, 17 = 14.71; p = 0.0013; two-way ANOVA; Fig. 2a-b). Moreover, frequency facilitation induced by 10 stimuli applied at frequencies ranging from 1 to 20 Hz is also significantly reduced at MF synapses of PS cDKO mice (1 Hz: F1, 13 = 11.64, p = 0.005; 5 Hz: F1, 13 = 13.33, p = 0.003; 10 Hz: F1, 15 = 9.67, p = 0.008; 20 Hz: F1, 15 = 9.71, p = 0.008; two-way ANOVA; Fig. 2c), providing further evidence for pre-synaptic short-term plasticity impairment in these mice. Thus, Presenilins are required for normal presynaptic short-term plasticity at hippocampal MF synapses.
Impaired post-tetanic potentiation at hippocampal MF synapses in PS cDKO mice
Other forms of short-term synaptic plasticity also include post-tetanic potentiation, which lasts seconds to several minutes and is longer-lasting than the time scale of hundreds of milliseconds for frequency facilitation. PTP is known to require mitochondrial Ca2+ for its induction [21, 22, 25, 26]. We examined PTP in the presence of APV (50 μM) and bicuculline (10 μM) at hippocampal MF synapses of PS cDKO and control mice using whole-cell patch clamp recording in CA3 pyramidal neurons. After baseline EPSC amplitudes were recorded for 5 min at 0.2 Hz, PTP was induced by high frequency stimulation (HFS: 16 pulses at 100 Hz, delivered 4 times at 0.33 Hz), and time-dependent changes in the EPSC amplitudes were measured. Figure 3a and b show representative time courses of the changes in normalized EPSC amplitudes relative to the baseline responses recorded from CA3 pyramidal neurons of control and PS cDKO mice. We found that PTP recorded in the MF pathway is reduced in CA3 pyramidal neurons of PS cDKO mice, relative to controls (Fig. 3c). Application of CGP37157 (20 μM), inhibitor of mitochondrial Ca2+ release via the Na+/Ca2+ exchanger (NCX), resulted in significant reduction of PTP at MF synapses of control mice, whereas CGP37157 treatment had little effect on PTP at MF synapses in PS cDKO mice (Fig. 3a-c). DCG IV (2 μM) was applied towards the end of the recording to confirm that MF synapses were recorded. These results show that PTP induction is impaired in the absence of Presenilins at MF synapses, and that blockade of mitochondrial Ca2+ release by CGP37157 in control mice mimics and occludes the PTP reduction in PS cDKO mice.
To confirm further whether synaptic inputs indeed arise from monosynaptic MF innervation, we next analyzed EPSC characteristics as previously reported [27, 28]. We found that synaptic latencies to the EPSC onset showed unimodal distribution and their range was 1.6–2.5 ms, with averages of 1.93 ± 0.03 and 2.01 ± 0.03 ms in control and PS cDKO mice, respectively (Fig. 3e). In addition, we measured kinetic parameters of EPSCs (10–90% rise time and decay time constant of EPSCs) to ensure that analysis was restricted to MF inputs. The mean 10–90% rise times are 2.27 ± 0.06 and 2.29 ± 0.05 ms in the range of 1.19–3.13 and 1.38–3.14 ms in control and PS cDKO mice, respectively (Fig. 3f). Furthermore, we found that the 10–90% decay time constant (τ) of EPSCs does not correlate with the EPSC amplitude (Fig. 3g). Taken together, these findings indicate that EPSC recordings in the MF pathway reflected monosynaptic responses.
Quantitative EM analysis of presynaptic MF boutons
Our findings showing that blockade of mitochondrial Ca2+ release in control mice mimics and occludes PTP impairment at MF synapses in PS cDKO mice suggest deficits in mitochondrial Ca2+ homeostasis in the absence of Presenilins. To determine whether mitochondrial content is altered at presynaptic MF boutons of PS cDKO mice, we performed quantitative EM analysis of PS cDKO and control mice at 2 months of age. MF synapses are known to exhibit unique ultrastructural characteristics compared to other hippocampal synapses, including large presynaptic boutons [29,30,31]. As shown in Fig. 4a, large numbers of mitochondria are present in presynaptic boutons of PS cDKO and control MF synapses. Quantitative analysis of mitochondrial profiles revealed similar numbers of mitochondria per bouton between control and PS cDKO mice (control: 10.02 ± 0.33, PS cDKO: 9.51 ± 0.33, n = 59 boutons, p > 0.05; Fig. 4b). Total area of mitochondria per bouton is also similar between control and PS cDKO MF synapses (control: 0.42 ± 0.04 μm2, n = 44 boutons; PS cDKO: 0.49 ± 0.04 μm2, n = 42 boutons, p > 0.05; Fig. 4c). Furthermore, the area of the presynaptic MF bouton is normal in PS cDKO mice (control: 6.04 ± 0.45 μm2, n = 59 boutons; PS cDKO: 6.41 ± 0.58 μm2, n = 42 boutons, p > 0.05; Fig. 4d). Thus, mitochondrial content is not changed at hippocampal MF presynaptic terminals in the absence of Presenilins.
Impaired mitochondrial Ca2+homeostasis in PS cDKO granule neurons
To evaluate Ca2+ homeostasis directly in DG granule neurons, which are the presynaptic neuron of the MF synapse, we used acute hippocampal slices to measure cytosolic Ca2+ concentration ([Ca2+]i) in DG granule neurons upon repeated stimulations at the same frequencies that were used to induce synaptic facilitation (Fig. 2c). We imaged the fluorescence of Fura-2 in the soma, which was introduced at a concentration of 100 μM via a whole-cell patch pipette (Fig. 5a). Before examining Ca2+ responses, we identified mature DG granule neurons in the hippocampus according to their electrophysiological criteria: low resting membrane potential (RMP) and input resistance (Ri), and high threshold current for action potential compared to young DG granule neurons [32, 33]. The mean values for RMP, Ri, and threshold currents for triggering action potential are similar between control and PS cDKO granule neurons (Fig. 5b-d; p > 0.05). Ca2+ transients were evoked by 10 repetitive stimulation (depolarizing pulses of 2 ms duration; from −80 to 0 mV) at varying frequencies (1, 5, 10, and 20 Hz) under voltage-clamp conditions. The resting [Ca2+]i is not significantly different between control (62.1 ± 4.1 nM; n = 16 neurons) and PS cDKO (82.9 ± 7.4 nM; n = 12 neurons, unpaired t-test, p = 0.102) DG neurons (Fig. 5e). However, the magnitude of [Ca2+]i changes (∆[Ca2+]i) elicited by 10 repetitive stimulation at 5, 10 and 20 Hz are significantly reduced in DG granule neurons of PS cDKO mice, compared to the control (*p < 0.05, **p < 0.01; Fig. 5f-g). These findings suggest that presynaptic Ca2+ deficits may contribute to or underlie the presynaptic facilitation impairment observed at MF synapses in PS cDKO mice (Fig. 2c).
To determine further whether the reduction of cytosolic Ca2+ increases in presynaptic neurons of MF synapses in PS cDKO mice is due to mitochondrial Ca2+ dysregulation, we examined the amplitude of [Ca2+]i changes elicited by repetitive stimulation in the absence or presence of CGP37157 (20 μM) at DG granule neurons of PS cDKO and control mice. We found that the magnitude of ∆[Ca2+]i induced by repetitive stimulation (10 depolarizing pulses of 2 ms duration; from −80 to 0 mV) at 20 Hz is significantly reduced in PS cDKO granule neurons, relative to the control (control: 360.1 ± 11.4 nM, PS cDKO: 250.7 ± 19.7 nM, unpaired t-test, p = 0.0003; Fig. 6a-b). In the presence of CGP37157, ∆[Ca2+]i in DG granule neurons of control mice is significantly reduced (control: 360.1 ± 11.4 nM, control + CGP: 289.2 ± 12.1 nM, paired t-test, p = 0.0008; Fig. 6a-b). However, CGP37157 treatment did not cause further significant reduction of ∆[Ca2+]i in DG granule neurons of PS cDKO mice (PS cDKO: 250.7 ± 19.7 nM, PS cDKO + CGP: 230.4 ± 22.2 nM, paired t-test, p = 0.482; Fig. 6a-b). Furthermore, ∆[Ca2+]i induced by the PTP induction protocol (16 pulses at 100 Hz, delivered 4 times at 0.33 Hz) is also significantly reduced in PS cDKO granule neurons, relative to the control (F1, 15 = 12.56, p = 0.0029; two-way ANOVA; Fig. 6c), and inhibition of mitochondrial Ca2+ release by CGP37157 significantly reduces the amplitude of ∆[Ca2+]i during PTP induction in control mice (F1, 14 = 28.46, p = 0.0001; two-way ANOVA), but does not significantly reduce ∆[Ca2+]i in PS cDKO mice (F1, 16 = 0.76, p = 0.40; two-way ANOVA; Fig. 6c). These results show that mitochondrial Ca2+ homeostasis is disrupted in the absence of Presenilins, and suggest that mitochondrial Ca2+ deficits in presynaptic DG granule neurons underlie the short-term plasticity impairment observed at MF synapses in PS cDKO mice.
Spatial memory impairments in PS cDKO mice
We further assessed PS cDKO and control mice in the Morris water maze using a difficult training protocol (4 trials a day; 13 days). The performance of both control and PS cDKO mice improved significantly during the course of training (day 1 vs. day 13, p < 0.001; Fig. 7a). Two-way ANOVA analysis revealed that PS cDKO mice exhibit significantly longer latencies (F1, 10 = 22.69, p < 0.001) and path lengths (F1, 10 = 9.62, p < 0.05) relative to control mice (Fig. 7a), while the swimming speed was similar (F1, 10 = 4.55, p > 0.05; data not shown). In the post-training probe trial on day 13, both control and PS cDKO mice searched preferentially in the target quadrant, but PS cDKO mice showed significantly reduced target quadrant occupancy (p < 0.01; Fig. 7b). These results demonstrate that PS cDKO mice exhibit profound spatial learning and memory impairment in the water maze.
The hippocampus is known to be particularly vulnerable in AD, and is composed of three major circuits [7,8,9, 17, 18]. Our previous studies of Presenilins and Nicastrin, another essential component of the γ-secretase complex, in synaptic function, however, focused exclusively on the hippocampal SC pathway [1, 2, 19, 34]. In the current study, we investigate the role of Presenilins at hippocampal MF synapses to determine whether Presenilins employ a universal or distinct mechanism to control synaptic function in the hippocampus. Our electrophysiological, quantitative EM and imaging analyses revealed the essential role of Presenilins in the regulation of synaptic plasticity and mitochondrial Ca2+ homeostasis at hippocampal MF synapses.
Similar to SC synapses, we found that presynaptic short-term plasticity, such as PPF and synaptic facilitation, and LTP are impaired at hippocampal MF synapses in the absence of Presenilins (Figs. 1 and 2), indicating a universal requirement of Presenilins for normal synaptic plasticity at the hippocampal SC and MF synapses. These findings are consistent with the spatial learning and memory deficits exhibited by these PS cDKO mice at 2 months of age in the hippocampal memory-dependent Morris water maze task using either an intensive training protocol (6 trials per day) in a prior study  or a less intensive and more difficult training protocol (4 trials per day) in the current study, which revealed more dramatic learning and memory deficits (Fig. 7). Interestingly, PS1 cKO mice also exhibited mild but significant learning and memory deficits using a similarly difficult training protocol, which was designed to uncover more readily spatial learning and memory impairment . Thus, the severity of learning and memory deficits observed in the water maze is Presenilin dose dependent with PS cDKO mice exhibit more severe phenotypes than PS1 cKO mice. The synaptic plasticity impairments observed in the MF pathway of PS cDKO mice in the current study and previously reported in the SC pathway [1, 2, 19] likely contribute to the spatial learning and memory deficits identified in the current and prior studies (Fig. 7, ). For example, MF synaptic plasticity was reported to be important for the establishment of hippocampus-dependent associative learning and spatial memory [35,36,37,38]. Furthermore, spatial learning and memory analyzed in the water maze results from network interactions between hippocampal tri-synaptic circuits and the entorhinal cortex. At 2 months of age, postnatal forebrain-restricted PS cDKO mice exhibit normal numbers of cortical and hippocampal neurons as well as normal volume of the neocortex and hippocampus, indicating unaffected cortical development in these mice [1, 3], despite neurodevelopment phenotypes observed in PS germ-line mutant mice and neural progenitor cell lineage restricted conditional mutant mice [39,40,41,42]. Future studies will be needed to determine whether and how Presenilins control synaptic plasticity in the hippocampal perforant path (PP).
The impairment in the LTP induction phase is more dramatic at MF synapses of PS cDKO mice (Fig. 1) than what was previously reported at SC synapses [2, 43]. This is likely due to the fact that high-frequency stimulation at MF synapses induces multiple forms of synaptic strength enhancements, including PTP, in LTP induction phase [44, 45]. Furthermore, in contrast to the SC and the perforant path, MF synapses display a particular form of LTP that is mainly expressed presynaptically, and is independent of NMDA receptor activation [45,46,47]. The early induction phase of LTP at MF synapses is triggered by a tetanus-induced rise in presynaptic intracellular Ca2+, which results in activation of a Ca2+/calmodulin-activated adenylyl cyclase [47,48,49,50]. The mitochondrial Ca2+ deficit observed in presynaptic neurons of the MF pathway in the absence of Presenilins (Fig. 6) likely underlies the greater impairment of early phase LTP induction at MF synapses relative to SC synapses.
Interestingly, we found that another form of presynaptic short-term plasticity, PTP, is impaired at MF synapses in PS cDKO mice (Fig. 3). Due to their unique structural features, CA3 pyramidal neurons receive excitatory synapses from stellate cells of layer II of the entorhinal cortex onto their distal apical dendrite [51, 52], and from other CA3 axon collaterals onto the remainder of the apical and the entire basal dendrite ; thus, the MF-CA3 projection may be contaminated with polysynaptic responses. We therefore performed whole-cell patch recording to ensure that the EPSCs recorded at MF synapses were monosynaptic. The latter is supported by the observations that the EPSC’s rise times are uniform, and their latencies are relatively short, and their distribution is unimodal (Fig. 3). Furthermore, if our EPSC recording were contaminated with polysynaptic contributions, then increasing the intensity of presynaptic stimulation would expect to result in slower-decaying synaptic currents. However, we found that the EPSCs decay time constant (τ) did not correlate with the EPSC amplitude or stimulation intensity (Fig. 3). This is consistent with monosynaptic nature of the recorded EPSCs [27, 28], and suggests that our EPSC recording in the MF pathway reflected monosynaptic responses with no significant contamination by polysynaptic components.
PTP is known to be dependent on mitochondrial Ca2+ and is longer lasting than frequency facilitation due to the slower release of Ca2+ from mitochondria [21, 22, 25, 54]. Indeed, blockade of mitochondrial Ca2+ release by NCX inhibitor CGP37157 mimics and occludes the PTP impairment observed at MF synapses of PS cDKO mice (Fig. 3), indicating that the PTP deficits in PS cDKO mice are due to the mitochondrial Ca2+ defects. However, quantitative EM analysis revealed similar number and area of mitochondria at presynaptic boutons of control and PS cDKO MF synapses (Fig. 4). Ca2+ imaging analysis of acute hippocampal slices demonstrated that Presenilins are essential for normal mitochondrial Ca2+ homeostasis at MF synapses (Figs. 5 and 6). We measured the ∆[Ca2+]i increments in the cell body of DG granule neurons instead of presynaptic axon terminals, and the cytosolic Ca2+ increases are reduced in DG granule neurons of PS cDKO mice when induced by tetanic stimulation between 5 and 20 Hz but unchanged at 1 Hz (Fig. 5). However, synaptic facilitation induced by repeated stimulation at 1, 5, 10 and 20 Hz is impaired at MF synapses of PS cDKO mice (Fig. 2). The difference between cytosolic Ca2+ increases and synaptic facilitation induced by repeated stimulation at 1 Hz is likely due to the fact that during stimulation [Ca2+]i increments are much higher in presynaptic axon terminals and have faster kinetics, compared to cell bodies, because of their different Ca2+ clearance mechanisms and endogenous Ca2+ buffers [55,56,57,58,59,60].
Blockade of mitochondrial Ca2+ release mimics the impairment of cytosolic Ca2+ increases elicited by PTP induction stimuli (16 pulses at 100 Hz, delivered 4 times) in DG granule neurons of PS cDKO mice (Fig. 6). Furthermore, the amplitude of cytosolic Ca2+ increases elicited by high frequency stimulation (>20 Hz) is similarly reduced in DG granule neurons of PS cDKO slices and in DG granule neurons of control slices treated with CGP37157, whereas CGP37157 has little effect in PS cDKO DG neurons (Fig. 6). These results suggest that the mitochondrial Ca2+ deficits likely contribute to the presynaptic impairment observed at MF synapses of PS cDKO mice. How Presenilins control mitochondrial Ca2+ homeostasis is unknown. We previously reported that ryanodine receptor (RyR)-mediated Ca2+ release from the ER is impaired in the absence of Presenilins [2, 61]. Furthermore, RyR levels are reduced in the hippocampus of PS cDKO mice but IP3 receptors and SERCA are unchanged . It remains to be determined whether Presenilin regulates mitochondrial homeostasis via its uniporter and/or antiporters or through its modulation of Ca2+ release from the ER, since communication between ER and mitochondrial membranes is thought to facilitate Ca2+ transfer [62,63,64]. Since mitochondrial Ca2+ dysregulation likely contributes to apoptotic neuronal death observed in PS cDKO mice during aging , future studies will aim at elucidation of the molecular mechanism by which Presenilins control mitochondrial Ca2+ homeostasis, which may be explored to prevent neurodegeneration caused by Presenilin dysfunction.
Our prior studies addressing the normal synaptic function of Presenilins and the dysfunction of Presenilin mutations all focused on the hippocampal Schaffer collateral pathway. Little is known about the function and dysfunction of Presenilins in other hippocampal synapses, such as the mossy fiber pathway, which are also vulnerable in the pathogenesis of Alzheimer’s disease. In this study, we report that loss of Presenilin function leads to impairment in long-term potentiation and multiple forms of presynaptic short-term plasticity at hippocampal mossy fiber synapses. Interestingly, mitochondrial Ca2+ homeostasis is also disrupted at mossy fiber synapses in the absence of Presenilin, though mitochondrial content is unaffected, and the presynaptic Ca2+ dysregulation likely contributes to the presynaptic impairment observed at mossy fiber synapses in PS cDKO mice. Our current study demonstrates the importance of Presenilin in the regulation of synaptic plasticity and mitochondrial Ca2+ homeostasis in the hippocampal mossy fiber pathway.
Excitatory postsynaptic currents
Field excitatory postsynaptic potentials
High frequency stimulation
- PS cDKO:
Presenilin conditional double knockout
- Ri :
Resting membrane potential
Sarcoendoplasmic reticulum Ca2+-ATPase
Theta burst stimulation
Saura CA, Choi SY, Beglopoulos V, Malkani S, Zhang D, Shankaranarayana Rao BS, et al. Loss of presenilin function causes impairments of memory and synaptic plasticity followed by age-dependent neurodegeneration. Neuron. 2004;42:23–36.
Zhang C, Wu B, Beglopoulos V, Wines-Samuelson M, Zhang D, Dragatsis I, et al. Presenilins are essential for regulating neurotransmitter release. Nature. 2009;460:632–6.
Wines-Samuelson M, Schulte EC, Smith MJ, Aoki C, Liu X, Kelleher RJ 3rd, et al. Characterization of age-dependent and progressive cortical neuronal degeneration in presenilin conditional mutant mice. PLoS One. 2010;5:e10195.
Hsia AY, Masliah E, McConlogue L, Yu GQ, Tatsuno G, Hu K, et al. Plaque-independent disruption of neural circuits in Alzheimer's disease mouse models. Proc Natl Acad Sci U S A. 1999;96:3228–33.
Cotman CW, Anderson KJ. Synaptic plasticity and functional stabilization in the hippocampal formation: possible role in Alzheimer's disease. Adv Neurol. 1988;47:313–35.
Santos SF, Pierrot N, Octave JN. Network excitability dysfunction in Alzheimer's disease: insights from in vitro and in vivo models. Rev Neurosci. 2010;21:153–71.
Braak H, Thal DR, Ghebremedhin E, Del Tredici K. Stages of the pathologic process in Alzheimer disease: age categories from 1 to 100 years. J Neuropathol Exp Neurol. 2011;70:960–9.
Gomez-Isla T, Price JL, McKeel DW Jr, Morris JC, Growdon JH, Hyman BT. Profound loss of layer II entorhinal cortex neurons occurs in very mild Alzheimer's disease. The Journal of neuroscience: the official journal of the Society for Neuroscience. 1996;16:4491–500.
Braak H, Braak E. Neuropathological stageing of Alzheimer-related changes. Acta Neuropathol. 1991;82:239–59.
Ally BA, Hussey EP, Ko PC, Molitor RJ. Pattern separation and pattern completion in Alzheimer's disease: evidence of rapid forgetting in amnestic mild cognitive impairment. Hippocampus. 2013;23:1246–58.
Fyhn M, Molden S, Witter MP, Moser EI, Moser MB. Spatial representation in the entorhinal cortex. Science. 2004;305:1258–64.
Lavenex P, Banta Lavenex P, Amaral DG. Postnatal development of the primate hippocampal formation. Dev Neurosci. 2007;29:179–92.
Andersen P, Bliss TV, Lomo T, Olsen LI, Skrede KK. Lamellar organization of hippocampal excitatory pathways. Acta Physiol Scand. 1969;76:4A–5A.
Kesner RP, Lee I, Gilbert P. A behavioral assessment of hippocampal function based on a subregional analysis. Rev Neurosci. 2004;15:333–51.
Okada K, Okaichi H. Functional differentiation and cooperation among the hippocampal subregions in rats to effect spatial memory processes. Behav Brain Res. 2009;200:181–91.
Rolls ET, Kesner RP. A computational theory of hippocampal function, and empirical tests of the theory. Prog Neurobiol. 2006;79:1–48.
Yassa MA, Stark SM, Bakker A, Albert MS, Gallagher M, Stark CE. High-resolution structural and functional MRI of hippocampal CA3 and dentate gyrus in patients with amnestic mild cognitive impairment. NeuroImage. 2010;51:1242–52.
Yassa MA, Lacy JW, Stark SM, Albert MS, Gallagher M, Stark CE. Pattern separation deficits associated with increased hippocampal CA3 and dentate gyrus activity in nondemented older adults. Hippocampus. 2011;21:968–79.
Zhang D, Zhang C, Ho A, Kirkwood A, Sudhof TC, Shen J. Inactivation of presenilins causes pre-synaptic impairment prior to post-synaptic dysfunction. J Neurochem. 2010;115:1215–21.
Yu H, Saura CA, Choi SY, Sun LD, Yang X, Handler M, et al. APP processing and synaptic plasticity in presenilin-1 conditional knockout mice. Neuron. 2001;31:713–26.
Tang Y, Zucker RS. Mitochondrial involvement in post-tetanic potentiation of synaptic transmission. Neuron. 1997;18:483–91.
Lee D, Lee KH, Ho WK, Lee SH. Target cell-specific involvement of presynaptic mitochondria in post-tetanic potentiation at hippocampal mossy fiber synapses. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2007;27:13603–13.
Steiner H, Duff K, Capell A, Romig H, Grim MG, Lincoln S, et al. A loss of function mutation of presenilin-2 interferes with amyloid beta-peptide production and notch signaling. J Biol Chem. 1999;274:28669–73.
Kamiya H, Shinozaki H, Yamamoto C. Activation of metabotropic glutamate receptor type 2/3 suppresses transmission at rat hippocampal mossy fibre synapses. J Physiol. 1996;493(Pt 2):447–55.
Kamiya H, Zucker RS. Residual Ca2+ and short-term synaptic plasticity. Nature. 1994;371:603–6.
Regehr WG, Delaney KR, Tank DW. The role of presynaptic calcium in short-term enhancement at the hippocampal mossy fiber synapse. The Journal of neuroscience: the official journal of the Society for Neuroscience. 1994;14:523–37.
Claiborne BJ, Xiang Z, Brown TH. Hippocampal circuitry complicates analysis of long-term potentiation in mossy fiber synapses. Hippocampus. 1993;3:115–21.
Toth K, Suares G, Lawrence JJ, Philips-Tansey E, McBain CJ. Differential mechanisms of transmission at three types of mossy fiber synapse. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2000;20:8279–89.
Blackstad TW, Kjaerheim A. Special axo-dendritic synapses in the hippocampal cortex: electron and light microscopic studies on the layer of mossy fibers. J Comp Neurol. 1961;117:133–59.
Hamlyn LH. The fine structure of the mossy fibre endings in the hippocampus of the rabbit. J Anat. 1962;96:112–20.
Rollenhagen A, Satzler K, Rodriguez EP, Jonas P, Frotscher M, Lubke JH. Structural determinants of transmission at large hippocampal mossy fiber synapses. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2007;27:10434–44.
Lee SH, Ho WK, Lee SH. Characterization of somatic Ca2+ clearance mechanisms in young and mature hippocampal granule cells. Cell Calcium. 2009;45:465–73.
Schmidt-Hieber C, Jonas P, Bischofberger J. Enhanced synaptic plasticity in newly generated granule cells of the adult hippocampus. Nature. 2004;429:184–7.
Lee SH, Sharma M, Sudhof TC, Shen J. Synaptic function of nicastrin in hippocampal neurons. Proc Natl Acad Sci U S A. 2014;111:8973–8.
Gruart A, Munoz MD, Delgado-Garcia JM. Involvement of the CA3-CA1 synapse in the acquisition of associative learning in behaving mice. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2006;26:1077–87.
Mitsuno K, Sasa M, Ishihara K, Ishikawa M, Kikuchi H. LTP of mossy fiber-stimulated potentials in CA3 during learning in rats. Physiol Behav. 1994;55:633–8.
Otto C, Kovalchuk Y, Wolfer DP, Gass P, Martin M, Zuschratter W, et al. Impairment of mossy fiber long-term potentiation and associative learning in pituitary adenylate cyclase activating polypeptide type I receptor-deficient mice. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2001;21:5520–7.
Wu ZL, Thomas SA, Villacres EC, Xia Z, Simmons ML, Chavkin C, et al. Altered behavior and long-term potentiation in type I adenylyl cyclase mutant mice. Proc Natl Acad Sci U S A. 1995;92:220–4.
Shen J, Bronson RT, Chen DF, Xia W, Selkoe DJ, Tonegawa S. Skeletal and CNS defects in Presenilin-1-deficient mice. Cell. 1997;89:629–39.
Handler M, Yang X, Shen J. Presenilin-1 regulates neuronal differentiation during neurogenesis. Development. 2000;127:2593–606.
Wines-Samuelson M, Handler M, Shen J. Role of presenilin-1 in cortical lamination and survival of Cajal-Retzius neurons. Dev Biol. 2005;277:332–46.
Kim WY, Shen J. Presenilins are required for maintenance of neural stem cells in the developing brain. Mol Neurodegener. 2008;3:2.
Saura CA, Chen G, Malkani S, Choi SY, Takahashi RH, Zhang D, et al. Conditional inactivation of presenilin 1 prevents amyloid accumulation and temporarily rescues contextual and spatial working memory impairments in amyloid precursor protein transgenic mice. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2005;25:6755–64.
Alle H, Jonas P, Geiger JR. PTP and LTP at a hippocampal mossy fiber-interneuron synapse. Proc Natl Acad Sci U S A. 2001;98:14708–13.
Zalutsky RA, Nicoll RA. Comparison of two forms of long-term potentiation in single hippocampal neurons. Science. 1990;248:1619–24.
Harris EW, Cotman CW. Long-term potentiation of guinea pig mossy fiber responses is not blocked by N-methyl D-aspartate antagonists. Neurosci Lett. 1986;70:132–7.
Nicoll RA, Malenka RC. Contrasting properties of two forms of long-term potentiation in the hippocampus. Nature. 1995;377:115–8.
Huang YY, Li XC, Kandel ER. cAMP contributes to mossy fiber LTP by initiating both a covalently mediated early phase and macromolecular synthesis-dependent late phase. Cell. 1994;79:69–79.
Nicoll RA, Schmitz D. Synaptic plasticity at hippocampal mossy fibre synapses. Nat Rev Neurosci. 2005;6:863–76.
Weisskopf MG, Castillo PE, Zalutsky RA, Nicoll RA. Mediation of hippocampal mossy fiber long-term potentiation by cyclic AMP. Science. 1994;265:1878–82.
Berzhanskaya J, Urban NN, Barrionuevo G. Electrophysiological and pharmacological characterization of the direct perforant path input to hippocampal area CA3. J Neurophysiol. 1998;79:2111–8.
Yeckel MF, Berger TW. Feedforward excitation of the hippocampus by afferents from the entorhinal cortex: redefinition of the role of the trisynaptic pathway. Proc Natl Acad Sci U S A. 1990;87:5832–6.
Li XG, Somogyi P, Ylinen A, Buzsaki G. The hippocampal CA3 network: an in vivo intracellular labeling study. J Comp Neurol. 1994;339:181–208.
Lee JS, Kim MH, Ho WK, Lee SH. Presynaptic release probability and readily releasable pool size are regulated by two independent mechanisms during posttetanic potentiation at the calyx of held synapse. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2008;28:7945–53.
Regehr WG. Interplay between sodium and calcium dynamics in granule cell presynaptic terminals. Biophys J. 1997;73:2476–88.
Reuter H, Porzig H. Localization and functional significance of the Na+/Ca2+ exchanger in presynaptic boutons of hippocampal cells in culture. Neuron. 1995;15:1077–84.
Usachev YM, DeMarco SJ, Campbell C, Strehler EE, Thayer SA. Bradykinin and ATP accelerate ca(2+) efflux from rat sensory neurons via protein kinase C and the plasma membrane ca(2+) pump isoform 4. Neuron. 2002;33:113–22.
Fierro L, DiPolo R, Llano I. Intracellular calcium clearance in Purkinje cell somata from rat cerebellar slices. J Physiol. 1998;510(Pt 2):499–512.
Kim MH, Lee SH, Park KH, Ho WK, Lee SH. Distribution of K+-dependent Na+/Ca2+ exchangers in the rat supraoptic magnocellular neuron is polarized to axon terminals. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2003;23:11673–80.
Suzuki S, Osanai M, Mitsumoto N, Akita T, Narita K, Kijima H, et al. Ca(2+)-dependent ca(2+) clearance via mitochondrial uptake and plasmalemmal extrusion in frog motor nerve terminals. J Neurophysiol. 2002;87:1816–23.
Wu B, Yamaguchi H, Lai FA, Shen J. Presenilins regulate calcium homeostasis and presynaptic function via ryanodine receptors in hippocampal neurons. Proc Natl Acad Sci U S A. 2013;110:15091–6.
Rizzuto R, Pinton P, Carrington W, Fay FS, Fogarty KE, Lifshitz LM, et al. Close contacts with the endoplasmic reticulum as determinants of mitochondrial Ca2+ responses. Science. 1998;280:1763–6.
Pivovarova NB, Pozzo-Miller LD, Hongpaisan J, Andrews SB. Correlated calcium uptake and release by mitochondria and endoplasmic reticulum of CA3 hippocampal dendrites after afferent synaptic stimulation. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2002;22:10653–61.
Giorgi C, De Stefani D, Bononi A, Rizzuto R, Pinton P. Structural and functional link between the mitochondrial network and the endoplasmic reticulum. Int J Biochem Cell Biol. 2009;41:1817–27.
We would like to thank H. Zhao for genotyping the mice, and the Shen lab members for helpful discussion.
This work was supported by grants from the National Institutes of Health (R01NS041783, R01NS042818 to J.S.) and the Deutsche Forschungsgemeinschaft (FR 620/14–1 to M.F.), and an award from the MetLife Foundation (to J.S.). M. Frotscher is a Senior Research Professor for Neuroscience of the Hertie Foundation.
Availability of data and materials
The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.
SHL performed all electrophysiology, imaging and behavioral experiments with assistance of MM, DL performed quantitative EM experiments, SHL, DL and MF analyzed the data. SHL, VYB, MF, and JS designed the experiments and wrote the paper. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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All animal studies were conducted in accordance with guidelines of the Brigham and Women’s Hospital Institutional Animal Care and Use Committee and National Institutes of Health.
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We dedicate this paper to the memory of Michael Frotscher, a generous and inspiring colleague and mentor.