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Measuring Synaptic Vesicle Endocytosis in Cultured Hippocampal Neurons

doi: 10.3791/55862 Published: September 4, 2017


Synaptic vesicle endocytosis is detected by light microscopy of pHluorin fused with synaptic vesicle protein and by electron microscopy of vesicle uptake.


During endocytosis, fused synaptic vesicles are retrieved at nerve terminals, allowing for vesicle recycling and thus the maintenance of synaptic transmission during repetitive nerve firing. Impaired endocytosis in pathological conditions leads to decreases in synaptic strength and brain functions. Here, we describe methods used to measure synaptic vesicle endocytosis at the mammalian hippocampal synapse in neuronal culture. We monitored synaptic vesicle protein endocytosis by fusing a synaptic vesicular membrane protein, including synaptophysin and VAMP2/synaptobrevin, at the vesicular lumenal side, with pHluorin, a pH-sensitive green fluorescent protein that increases its fluorescence intensity as the pH increases. During exocytosis, vesicular lumen pH increases, whereas during endocytosis vesicular lumen pH is re-acidified. Thus, an increase of pHluorin fluorescence intensity indicates fusion, whereas a decrease indicates endocytosis of the labelled synaptic vesicle protein. In addition to using the pHluorin imaging method to record endocytosis, we monitored vesicular membrane endocytosis by electron microscopy (EM) measurements of Horseradish peroxidase (HRP) uptake by vesicles. Finally, we monitored the formation of nerve terminal membrane pits at various times after high potassium-induced depolarization. The time course of HRP uptake and membrane pit formation indicates the time course of endocytosis.


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Neurotransmitters are stored in synaptic vesicles and released by exocytosis. The synaptic vesicle membrane and protein are then internalized by endocytosis, and reused in the next round of exocytosis. Endocytosis of synaptic vesicles is important for maintaining synaptic vesicle pools and removes protruding vesicles from the plasma membrane. The pH-sensitive green fluorescent protein pHluorin, which is quenched in acidic circumstances and dequenched in neutral pH, has been used to measure endocytosis time courses in live cells1,2,3. The pHluorin protein is typically attached to the lumenal side of synaptic vesicle proteins, such as synaptophysin or VAMP2/synaptobrevin. At rest, pHluorin is quenched in the 5.5 pH lumen of synaptic vesicles. Vesicle fusion to the plasma membrane exposes the vesicular lumen to the extracellular solution where the pH is ~7.3, resulting in an increase in pHluorin fluorescence. After exocytosis, the increased fluorescence decays, due to endocytosis of synaptic vesicle proteins followed by vesicle re-acidification within those recovered vesicles. Although the decay reflects both endocytosis and vesicular re-acidification, it mostly reflects endocytosis, because re-acidification is faster than endocytosis in most conditions1,4. The time constant of re-acidification is 3-4 s or less5,6, which is generally faster than the 10 s or more required for vesicle endocytosis4,5. If experiments are needed to distinguish endocytosis from re-acidification, acid quenching experiments using the 4-Morpholineethanesulfonic acid (MES) solution (25 mM) with a pH of 5.5 can be used to determine whether synaptic vesicle proteins are retrieved from the plasma membrane via endocytosis1,3,4. Thus, the pHluorin fluorescence intensity increase reflects a balance of exo- and endocytosis, and the decrease after nerve stimulation specifically reflects endocytosis.

pHluorin imaging may be used not only to measure the time course of endocytosis, but also the size of synaptic vesicle pools7,8, and the probability of evoked release and spontaneous release9. Many factors and proteins involved in regulating endocytosis, such as calcium, soluble NSF-attachment protein receptor (SNARE) proteins, brain-derived neurotrophic factor(BDNF), and calcineurin have been identified using pHluorin imaging1,2,10,11,12,13,14,15,16. Moreover, release of neurotransmitter could be detected in not only primary neurons but in neuroblastoma cells with TIRFM17. Recently, pHluorin variants, dsRed, mOrange and pHTomato were developed for monitoring simultaneous recordings of multiple factors in a single synapse18,19. For example, pHTomato has been fused with synaptophysin and used with a genetically encoded calcium indicator (GCaMP5K) to monitor presynaptic vesicle fusion and Ca2+ influx in the postsynaptic compartment20. Therefore, pHluorin attached to synaptic proteins provides a useful method to analyze the relationship between endocytosis and exocytosis.

EM is another method commonly used to study endocytosis, due to the high spatial resolution that shows ultrastructural changes during endocytosis. Two general areas are the ability to visualize pathological changes within neuronal cells21 and track vesicle proteins22. In particular, the observation of synaptic vesicle uptake, membrane curvature coated by clathrin in the periactive zone, and endosomal structures are possible with EM3,23,24,25,26,27,28. While EM involves potential artifacts, such as fixative-induced malformations, that may affect endocytosis, and data analysis is labor intensive, the resolution provides an attractive opportunity to visualize cellular structure. Potential fixative problems and the limitation in EM temporal resolution can be overcome by high pressure freezing, providing a fast and non-chemical method of stabilizing the delicate structures present during endocytosis27.

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NOTE: The following protocol describes the pHluorin imaging methods and EM methods used in cultured hippocampal neurons. pHluorin monitors synaptic vesicle protein uptake in living cells and EM detects uptake of synaptic vesicle and ultrastructural changes.

Animal care and procedure followed NIH guidelines and were approved by the NIH Animal Care and Use Committee.

1. pHluorin Imaging

  1. Hippocampal neuron culture
    1. Prepare Hippocampus Buffer (HB) by combining 4 mM NaHCO3 and 5 mM HEPES and adjust to pH 7.3 with 5 M NaOH. Make the culture medium by mixing neurobasal medium, 2% B27, 0.5 mM L-glutamine and 1% penicillin-streptomycin. Additionally, prepare a mixture of HB buffer with 20% Fetal Bovine Serum (HB/20% FBS).
      NOTE: This culturing protocol is based on Sankaranarayanan, et al.29 and Wu, et al.24
    2. Decapitate mouse pups between postnatal day 0 to day 2 into culture medium, and extract the brain into 4 °C HB/20% FBS. Remove the brainstem and thalamus to expose the hippocampi. Dissect out the hippocampi, after exposing it by removal of the brainstem and thalamus, and transfer to fresh 4 °C HB/20% FBS.
      NOTE: Typically, yield is around 4 x 105 cells/mL for one pup (two hippocampi). Clean off the adhering membranes using tweezers or scissors, then transfer to fresh 4 °C HB/20% FBS. Unroll the dentate gyrus and isolate the subiculum by cutting with scissors, then transfer to fresh 4 °C HB/20% FBS.
    3. Divide each hippocampus, by cutting from end to end, into about 10 slices and transfer them to a 15 mL polypropylene conical tube.
    4. After allowing the tissue to settle, wash with 10 mL of HB/20% FBS, and then wash three times with 10 mL of HB.
    5. Prepare digestion solution of 137 mM NaCl, 5 mM KCl, 7 mM Na2HPO4, and 25 mM HEPES, and adjust to pH 7.2 with 5 M NaOH. Remove the supernatant from the hippocampi. Add 10 mg of trypsin and 1 mg of DNase to 2 mL of digestion solution, and filter through a sterile 0.22 µm membrane directly onto the sample pellet.
    6. Incubate the hippocampi for 5 min at 37 °C, then wash twice with 10 mL of HB/20% FBS, and then wash once with 10 mL of HB.
    7. Dissociate the cells with 6 mg of MgSO4∙7H2O and 1 mg of DNase to 2 mL HB and sterile filter onto the hippocampi pellet through a sterile 0.22 µm filter. Gently dissociate the cells by careful triturating, while taking care to avoid introducing air bubbles. Allow tissue particulates to settle for 2 min, and then slowly transfer the supernatant to another tube.
    8. Add 3 mL HB/20% FBS to the cell suspension, and centrifuge or 10 min at 4 °C and 1,000 rpm. Discard the supernatant and resuspend in culture medium.
    9. Plate 60,000 cells suspended in 150 µL culture medium on a Poly-D-Lysine coated 25-mm diameter coverslip, without spill off the coverslip. Add 2 mL of pre-warmed culture medium 2 h after plating. Coverslips are maintained in 6-well culturing plates or sterile Petri dishes.
    10. Maintain cells at 37 °C in a 5% CO2 humidified incubator in culture medium for 14-21 days prior to recording. During the culture growth, change the top half of the medium twice a week.
  2. Transfection
    1. 6-7 days after plating, transfect synaptophysin-pHluorin 2X (SpH) or VAMP2-pHluorin into hippocampal neurons. For SpH, use a Cytomegalovirus (CMV) promoter, inserted into a pcDNA3 vector30. For VAMP2-pHluorin, use a CMV promoter inserted into a pCI vector31.
    2. Transfect either vector by lipid carrier into target cells, using 1 µg of plasmid. Use culture medium from protocol step 1.1.1, which lacks serum, for the transfection. Change the medium 2 h after transfection to reduce toxicity.
      NOTE: In case of low expression of SpH in the boutons, increase the DNA concentration to 2 µg or the incubation time with the lipid carrier, unless the cells are unhealthy. Typically, 4-10 cells (0.006-0.008%) of neurons were transfected.
  3. Light microscopy
    1. Prepare normal saline solution composed of 119 mM NaCl, 2 mM CaCl2, 2.5 mM KCl, 25 mM HEPES (pH 7.4), 30 mM glucose, 2 mM MgCl2, 0.01 mM 6-cyano-7-nitroquinoxaline-2,3-dione (CNQX), and 0.05 mM DL-2-amino-5-phosphonovaleric acid (AP5). Take a coverslip from the culture medium plate and place on an imaging chamber that allows field stimulation, using lubricant and sealant to avoid leaks. Avoid letting the glass dry during the transfer of a coverslip from the plate to the chamber by immediately adding 750 µL normal saline solution.
      NOTE: CNQX and AP5 were used to block postsynaptic activity, which has the potential for recurrent activity. Before placing a chamber on an inverted fluorescence microscope, use cleaning tissue to confirm that the chamber does not leak. Slow leaking causes focus changes during the recording by the mixing of normal saline and immersion oil, which results in changes in the refractive index.
    2. Stimulation and recording
      1. Image on an inverted widefield microscope with a 60X (1.4 numerical aperture) oil immersion lens with a metal halide lamp. Visualize pHluorin with a filter set for an excitation peak of 480 nm, a 490 nm long pass mirror, a 500-550 nm emission filter, and a manual flip shutter. Capture images every 100 ms, with 2 x 2 binning, using an Electron Multiplying Charge Coupled Device (EMCCD) camera.
        NOTE: Several features should be considered to achieve the proper conditions to avoid photobleaching, including the image capture interval, and filter and binning, which are dependent on equipment. In the case of confocal imaging, laser power and exposure time should be considered to avoid photobleaching. The setup was determined after recording at least 3 min without stimulus and the recording was performed for at least 10 s without stimulus to check for photobleaching.
      2. Choose an area with a high density of boutons for ease of analysis in each experiment. Identify transfected cells by their green fluorescence signal, with emphasis on round or oval expression patterns in the bouton and continuous expression between boutons.
      3. Induce endocytosis by field stimulation using a 1 ms pulse, 20 mA action potential (AP) supplied from a pulse stimulator and delivered through a platinum electrode within the stimulus isolation unit. Image fluorescence activity over the course of the stimulation and during cell recovery.
        NOTE: In the case of dead cells, expression was stronger than living boutons and showed a patchy pattern between boutons.
  4. Image analysis
    1. For analyzing the fluorescence intensity in a single bouton, set up a Region of Interest (ROI) as a 1.5 x 1.5 µm square; the size of a bouton is within about 1.5 µm. Use traces prior to stimulation to check for photobleaching and subtract as background.
    2. Normalize fluorescence change (ΔF) with the equation: Equation
      where Fmax and F0 refer to maximal increase after stimulation and baseline fluorescence, respectively. Measure endocytosis rates as the rate of decay during the first 4-10 s after the maximum point of pHluorin fluorescence. Obtain the time constant (τ) of endocytosis by fitting the pHluorin fluorescence decay from the peak increase to the baseline with a mono-exponential function.

2. Electron Microscopy

  1. Prepare a Poly-D-Lysine coated 6-well plate by applying 1.5 mL of 0.01% sterile-filtered Poly-D-Lysine solution to each well for 1 h at room temperature, then washing three times with sterilized water. Dissect, culture, and maintain hippocampal neurons as in steps 1.1.1, 1.1.2, and 1.1.3, respectively.
  2. Prepare a high K+ stimulation solution with HRP as 31.5 mM NaCl, 2 mM CaCl2, 90 mM KCl, 25 mM HEPES (pH 7.4), 30 mM glucose, 2 mM MgCl2, 0.01 mM CNQX, 0.05 mM AP5, and 5 mg/mL HRP, then adjust to pH 7.4 with 5 M NaOH.
    1. Stimulate the hippocampal neuron culture with 1.5 mL high K+ stimulation solution at room temperature (referred to as K+) by addition of 1.5 mL to each well for 90 s. In the resting condition (referred to as R), apply the same concentration of 5 mg/mL HRP for 90 s, but with normal saline solution. For the recovery sample, apply high K+ stimulation solution as with the K+ sample, then rapidly wash and replace with normal saline and incubate for 10 min.
  3. Fixation and staining
    1. Prepare 0.1 M Na cacodylate buffer using 21.4 g/L Na cacodylate at pH 7.4. Fix cells with 4% glutaraldehyde in 0.1 M Na cacodylate buffer for at least 1 h at room temperature. Wash three times with 0.1 M Na cacodylate buffer for 7 min each.
    2. Prepare Diaminobenzidine (DAB) solution, comprised of 0.5 mg/mL of DAB with 0.3% H2O2 in ddH2O, and filter with a 0.22 µm filter. Apply 1.5 mL DAB solution for 30 min at 37 °C. Wash three times with 0.1 M Na cacodylate buffer for 7 min each.
      CAUTION: DAB is a toxic and suspected carcinogen. Please use gloves and lab coats.
      NOTE: Labeling with DAB occurs due to its oxidation by H2O2, as catalyzed by HRP. Small increases in the components result in an increased signal in the sample. Increasing the concentration of HRP speeds up the effect of the catalyst. Sufficiently large concentrations of H2O2 allow for debilitating side reactions with HRP, inhibiting the effect of labeling32. In this work, the concentrations of this labeling system were chosen based on currently available research33,34.
    3. Incubate the neurons with 1.5 mL of 1% OsO4 in 0.1 M Na cacodylate buffer for 1 h at 4 °C as post fixation. Wash three times with 1.5 mL of 0.1 M Na cacodylate buffer for 7 min each.
      CAUTION: Due to the toxicity and reactivity of OsO4, keeping the sample on ice in a chemical hood is preferable in many cases to using a fridge for the incubation.
    4. Prepare 0.1 M sodium acetate buffer with 13.61 g/L sodium acetate and 11.43 mL/L glacial acetic acid at pH 5.0. Wash three times with 1.5 mL 0.1 M acetate buffer at pH 5.0 for 7 min each and incubate with 1.5 mL 1% uranyl acetate in 0.1 M acetate buffer at pH 5.0 for 1 h at 4 °C. Wash three times with 1.5 mL 0.1 M acetate buffer for 7 min each.
  4. Epoxy embedding
    1. Dehydrate the neuron culture with single 1.5 mL washes of 50%, 70%, and 90% ethanol, for 7 min in each and then 3 washes of 1.5 mL 100% ethanol for 7 min each in a fume hood.
    2. Mix 485 mL/L bisphenol-A-(epichlorhydrin) epoxy resin, 160 mL/L dodecenyl succinic anhydride (DDSA), 340 mL/L Methyl-5-Norbornene-2,3-Dicarboxylic Anhydride (NMA), and 15 mL/L 2,4,6-tris(dimethylaminomethyl)phenol (DMP-30) to create the epoxy resin. Mix thoroughly, then store under vacuum to remove air bubbles.
      NOTE: It is critical to remove air bubbles in the resin, especially those smaller than visible to the naked eye, because they can cause cavities in the resin during sectioning.
    3. Infiltrate the sample by replacing the ethanol with 50% epoxy resin in ethanol for 30 min at room temperature on a shaker, then 70% epoxy resin in ethanol for 30 min at room temperature on a shaker.
    4. Switch the epoxy resin solution with 100% epoxy resin and incubate for 10 min at 50 °C. Perform two exchanges of fresh 100% epoxy resin with incubations for 1 h at 50 °C. Add fresh 100% epoxy resin and allow to harden at 50 °C overnight and then at 60 °C for over 36 h to harden.
  5. Remove each sample from the muti-well plate with a jeweler's handsaw. Select regions of interest, dense concentrations of cells, using an inverted light microscope, and then cut 70 to 80 nm blocks for sectioning by microtome. Mount the cut region in the microtome chuck and load the microtome. Position the chuck in the microtome and mount a diamond knife with the edge parallel to the surface of the block. Collect sections of 70 to 80 nm thickness directly onto individual grids.
  6. Dissolve uranyl acetate into water for a 1% solution by weight, and separately dissolve lead citrate into water for a 3% solution by weight. Counterstain the sections by submersion with 1% aqueous uranyl acetate for 15 min and then 3% aqueous lead citrate for 5 min to improve the contrast of the samples.
  7. EM imaging
    1. Examine the sections with a transmission electron microscope and record images with a CCD digital camera at a primary magnification of 10,000-20,000X3.
  8. Statistics
    1. Perform a t-test to identify significant differences by comparing the mean and standard error of measurement (s.e.m.) between the control and experimental samples.

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Representative Results

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Using the lipid carrier method, SpH was expressed in hippocampal neurons, allowing for the identification of boutons (Figure 1a). Electrical stimulation of the cells induced exocytosis, and a corresponding increase in fluorescence intensity. The increase in fluorescence (ΔF) was stopped by ending the stimulus (Figure 1b). The increased fluorescence was followed by a slow decrease, due to endocytosis. In the case of VAMP2-pHluorin, VAMP2 diffuses along the axon from a bouton after stimulus4. The raw data used arbitrary units, and was normalized to the baseline to obtain the rate of decay and τ (Figure 2a-c). Since the measurements were made from a normalized trace, the rate of decay reflects the initial decay of fluorescence in the percentage of the peak ΔF per second (ΔF/s). In our experimental conditions, endocytosis (usually longer than 10 s) was much slower than reacidification (~3-4 s)4,5. Thus, the fluorescence decay of pHluorin primarily reflects endocytosis4,5. In presynaptic boutons, ΔF is larger than the axon except bouton and the beginning time-of-increase was matched with initiation of electrical stimulus. In axon except bouton, ΔF was lower in comparison to regions with boutons and beginning time-of-increase was delayed compared to the initiation of electrical stimulus (Figure 2b). ΔF induced in bouton and axon except bouton was 82.9 ± 9.0% (n = 5 experiments) and 23.2 ± 4.0% (n = 5 experiments), respectively (Figure 2b). ΔF of SpH decayed mono-exponentially with a τ of 17.7 ± 0.3 (n = 5 experiments) and 20.7 ± 0.2 (n = 4 experiments) in 50 AP and 200 AP, respectively (Figure 1b). In 200 AP, τ was not significantly different before or after normalizing with the baseline. In the case of VAMP2-pHluorin transfected cells, the expression level of VAMP2-pHluorin was higher than SpH (Figure 3a-c). Traces of VAMP2-pHluorin were also obtained by normalizing to the baseline (Figure 3b).

EM was performed in cultured neurons and the clathrin coated vesicles were examined in comparison to control samples, which were incubated with 5 mg/mL of HRP for 90 s in absence of the stimulus (Figure 4a-b). The clathrin coated pits were observed at a probability of 0.05 per bouton in the absence of stimulus. Stimulation with high K+ induced bulk endosome and synaptic vesicles uptake, which were identified by HRP labeling (Figure 5a). Synaptic vesicles were defined as vesicles with a diameter less than 50 nm and bulk endosomes were defined as having a diameter over 80 nm or with a cross sectional area of more than an 80 nm vesicle. Induced bulk endosome uptake was decreased by recovery with normal saline (Figure 5b).

Figure 1
Figure 1: Images of SpH transfected neurons and traces of SpH transfected cell responses to electrical stimulation. (a) A sample image of cultured hippocampal neurons transfected with SpH by liposome delivery. SpH was highly expressed in boutons, presenting circle or oval patterns, with relatively lower expression along the axon. White boxes indicate ROI containing boutons (1.5 x 1.5 µm). Scale bar: 20 µm. (b) Responses of SpH transfected cells to an electrical stimulus of 50 AP at 20 Hz (n = 5 experiments) or 200 AP at 20 Hz (n = 4 experiments). Each experiment was based on 20-60 boutons. Please click here to view a larger version of this figure.

Figure 2
Figure 2: Rate of decay and tau value for endocytosis. (a) Responses to 50 AP at 20 Hz were converted from arbitrary units to normalized traces (n = 5). Fluorescence change was normalized to the baseline. This figure has been modified from Wu et al., 20163. (b) Normalized responses to 200 AP at 20 Hz in boutons (black, n = 4 experiments, left panel) and axon except bouton (red, n = 4 experiments, left panel). Fluorescence change was normalized to the baseline. Dashed box is magnified in the right panel. (c) Using normalized baseline, the rate of decay or τ was calculated in 50 AP (n = 5 experiments) and 200 AP (n = 4 experiments) at 20 Hz. Before calculation, ΔF was normalized to 100%. τ of endocytosis was obtained from normalized trace between the time of maximum fluorescence and the end of experiment. Rate of decay (mean + s.e.m., upper panel) and τ (mean + s.e.m., lower panel) induced by 50 AP and 200 AP.  Please click here to view a larger version of this figure.

Figure 3
Figure 3: Images of VAMP2-pHluorin transfected neurons and examples of traces. (a) A sample image of cultured hippocampal neurons transfected with VAMP2-pHluorin by liposome delivery. White boxes indicate the ROI containing boutons (1.5 x 1.5 µm). Scale bar: 20 µm. (b) Traces for VAMP2-pHluorin responses to 200 AP at 20 Hz (n = 4 experiments). Fluorescence change was normalized to the baseline. (c) Fbase (a.u.) (mean + s.e.m.) in VAMP2-pHluorin (n = 4 experiments) and SpH (n = 7 experiments) transfected boutons. **, p <0.01. Please click here to view a larger version of this figure.

Figure 4
Figure 4: Images of EM in presynaptic terminal. (a) Synaptic vesicles were shown in cultured hippocampal neurons using EM. This figure has been modified from Wu et al., 20163. Scale bar = 200 nm. (b) Magnified image showing clathrin coated pits. Scale bar: 50 nm. Please click here to view a larger version of this figure.

Figure 5
Figure 5: Images of presynaptic terminal in stimulated neurons with high potassium. (a) EM images of neurons. The cells were fixed without stimulus (R), immediately after stimulation with 90 mM KCl for 90 s containing soluble HRP (K+), or after stimulation and then incubated for 10 min in normal saline. This figure has been modified from Wu et al., 20163. Scale bar = 200 nm. (b) Compared to control, HRP (-) synaptic vesicles were decreased and HRP (+) vesicles were increased by KCl. Bulk endosome uptake was induced by KCl and gradually decreased by recovery (mean + s.e.m., each group was from 40-100 synaptic profiles). *p <0.1; **p <0.01, significant to resting; ##p <0.01, significant to K+. Please click here to view a larger version of this figure.

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Here we demonstrate two methods for monitoring synaptic vesicle endocytosis. In the first method, we monitored pHluorin fused with a synaptic vesicle protein in transfected neurons and subsequently electrically stimulated. Secondly, we used EM imaging of HRP uptake as induced by KCl. We used different stimuli for two reasons. First, high potassium application induces depolarization of all neurons in the culture. This facilitates EM examination, given that our EM methodology could not distinguish between non-stimulated and stimulated neurons. Second, ultra-structural morphological changes were more reliably observed after intense stimulation, such as the high potassium stimulation, whereas pHluorin fluorescence changes can be observed after a brief train of action potentials or even a single action potential.

Light microscopy imaging using pHluorin shows synaptic vesicle protein fusion and uptake with high temporal resolution in living cells. It can be used to study mechanisms that regulate the endocytosis time course and the size of synaptic vesicle pools. pHluorin imaging has not only been used for monitoring synaptic protein endocytosis, but also for monitoring evoked or spontaneous single vesicle release, short-term synaptic plasticity, and for the measurement of the release probability35. Using pHluorin has shown that the synaptic vesicular protein pools being released are not the same as those being retrieved36,37. Recently, pHluorin fused with synaptic proteins was used to detect the fate of newly fused vesicles38, and bulk endocytosis39. Therefore, pHluorin fused with a synaptic protein is a valuable tool for studying exocytosis and endocytosis in living synapses.

The limitation of this technique is that the decay of the fluorescence intensity reflects not only endosomes, but also vesicular re-acidification. These two components could potentially be separated by treatment with bafilomycin, an inhibitor of V-ATPase10,40. Moreover, the fluorescence increase during electrical stimulation reflects the net outcome of exocytosis and endocytosis. Although pHluorin imaging could not detect membrane invagination, this limitation can be overcome by other techniques, particularly EM.

In EM, strongly stimulated cells showed increased HRP-positive synaptic vesicles and bulk endosomes. These bulk endosomes gradually disappeared by then regenerating into synaptic vesicles24. This technique shows synaptic vesicle uptake by revealing the ultrastructure in the presynaptic terminal in both control and stimulated cells. A drawback to this technique is assessing synaptic vesicle uptake in fixed cells rather than living cells. Additionally, the possibility of a fixative induced artifact cannot be excluded. Known artifacts affecting the membrane include blebbing, membrane erosion, and protein changes41. These differences from the naturally occurring state of a cell are an inherent concern to all methods of visualizing cells, and particular attention was paid to the EM data presented to assess the possibility of such artifacts41,42,43. While this technique alone cannot show functional endocytosis of synaptic proteins, combining it with light microscopy, which can provide live images of the endocytosis process, creates a more complete view of this cellular mechanism.

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The authors have nothing to disclose.


We thank Dr. Yong-Ling Zhu for providing synaptophysin-pHluorin2x construct, and Dr. James E. Rothman for providing VAMP2-phluorin. We thank Dr. Susan Cheng and Virginia Crocker of NINDS Electron Microscopy Facility for their technical support and help. This work was supported by the National Institute of Neurological Disorders and Stroke Intramural Research Program in USA and a grant from the KRIBB Research Initiative Program (Korean Biomedical Scientist Fellowship Program), Korea Research Institute of Bioscience and Biotechnology, Republic of Korea.


Name Company Catalog Number Comments
Lipofectamine LTX with Plus Thermo Fisher 15338-100 Transfection of plasmid DNA including synaptophysin or VAMP2-pHluorin
neurobasal medium Thermo Fisher 21103-049 Growth medium for neuron, Warm up to 37°C before use
B27 Thermo Fisher 17504-044 Gradient for neuronal differentiation
Glutamax Thermo Fisher 35050-061 Gradient for neuronal culture
Poly-D-Lysine coated coverslip Neuvitro GG-25-pdl Substrate for neuronal growth and imaging of pHluorin
Trypsin XI from bovine pancrease Sigma T1005 Neuronal culture-digest hippocampal tissues
Deoxyribonuclease I from bovine pancreas Sigma D5025 Neuronal culture-inhibits viscous cell suspension
pulse stimulator A-M systems model 2100 Apply electrical stimulation
Slotted bath with field stimulation Warner Instruments RC-21BRFS Apply electrical stimulation
stimulus isolation unit Warner Instruments SIU102 Apply electrical stimulation
lubricant Dow corning 111 pHluorin imaging-seal with coverslip and imaging chamber, avoid leak from chamber
AP5 Tocris 3693 Gradient for normal saline, selective NMDA receptor antagonist, inhibit postsynaptic activity which have potential for recurrent activity
CNQX Tocris 190 Gradient for normal saline, competitive AMPA/kainate receptor antagonist, inhibit postsynaptic activity which have potential for recurrent activity
Illuminator Nikon C-HGFI Metal halide light source for pHluorin
EMCCD camera Andor iXon3 pHluorin imaging, detect pHluorin fluorescence intensity
Inverted microscopy Nikon Ti-E Imaging for synaptophysin or VAMP2 pHluorin transfected cells
NIS-Elements AR Nikon NIS-Elements Advanced Research Software for imaging acquisition and analysis
Igor Pro WaveMetrics Igor pro Software for imaging analysis and data presentation
imaging chamber Warner Instruments RC21B pHluorin imaging, apply field stimulation on living cells
poly-l-lysine Sigma P4832 Electron microscopy, substrate for neuronal growth, apply on multiwell plate for 1 h at room temperature then wash with sterilized water 3 times
Horseradish peroxidase(HRP) Sigma P6782 Electron microscopy, labeling of endocytosed synaptic vesicles by catalyzing DAB in presence hydrogen peroxide, final concentration is 5 mg/mL in normal saline, make fresh before use
Na cacodylate Electron Microscopy Sciences 12300 Electron microscopy, buffer for fixatives and washing, final concentration is 0.1 N
3,3′-Diaminobenzidine(DAB) Sigma D8001 Electron microscopy, labeling of endocytosed synaptic vesicles, substrate for HRP, final concentration is 0.5 mg/mL in DDW and filtered, make fresh before use
Hydrogen peroxide solution Sigma H1009 Electron microscopy, labeling of endocytosed synaptic vesicles by inducing HRP-DAB reaction, final concentration is 0.3% in DDW, make fresh before use
glutaraldehyde Electron Microscopy Sciences 16365 Electron microscopy, fixatives, final concentration is 4% in Na-cacodylate buffer, make fresh before use, shake well before to use
TEM JEOL 200CX Electron microscopy, imaging of endocytosed vesicles and ultrastructural changes
CCD digital camera AMT XR-100 Electron microscopy, capturing images
Lead citrate Leica microsystems 16707235 Electron microscopy, grid staining



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Measuring Synaptic Vesicle Endocytosis in Cultured Hippocampal Neurons
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Villarreal, S., Lee, S. H., Wu, L. G. Measuring Synaptic Vesicle Endocytosis in Cultured Hippocampal Neurons. J. Vis. Exp. (127), e55862, doi:10.3791/55862 (2017).More

Villarreal, S., Lee, S. H., Wu, L. G. Measuring Synaptic Vesicle Endocytosis in Cultured Hippocampal Neurons. J. Vis. Exp. (127), e55862, doi:10.3791/55862 (2017).

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