The authors would like to thank the Swedish Research Council (349-2007-8680) for funding and Dalsj&#246;fors K&#246;tt AB (Dalsj&#246;fors, Sweden) for donation of bovine adrenal glands.

1. Cell Culture of Bovine Chromaffin Cells Isolated by Enzymatic Digestion from Adrenal Glands
<ol>
	<li>To isolate chromaffin cells collected from bovine adrenal glands, sterilize cells with 70% ethanol solution. Trim away fat and connective tissue using a scalpel. To remove blood, rinse the adrenal veins using Locke&#39;s solution (NaCl 154 mM, KCl 5.6 mM, NaHCO3 3.6 mM, hydroxyethyl piperazineethanesulfonic acid (HEPES) 5.6 mM at pH 7.4) that has been thermostated to 37 &#176;C.</li>
	<li>To digest the tissue, inflate each gland by injecting approximately 2.5 mL of warm sterile-filtered 0.2% collagenase P solution through the adrenal vein using a syringe and incubate the tissue for 20 min at 37 &#176;C. Examine the glands to ensure the digestion process of the medulla is completed. The tissue should feel soft and not tense.</li>
	<li>Collect the digested medulla by snipping off the glands in the longitudinal direction. Mince the medulla tissue using a scalpel. Filter the tissue suspension over a steel sieve and dilute with Locke&#39;s solution to approximately a 50 mL volume to reduce the activity of collagenase P.</li>
	<li>Pellet the cells at 300 x g in a centrifuge for 10 min at room temperature and collect into 50 mL sterile test tubes. Re-suspend the obtained pellet in 20 mL Locke&#39;s solution and filter the solution over a sterile 100-&#181;m nylon mesh into tubes.</li>
	<li>Mix the chromaffin cell suspension with sterile Percoll (1:1) and centrifuge the cell solution at 18,600 x g for 20 min at room temperature. Collect the top layer of the density gradient and filter the solution over a 100-&#181;m nylon mesh into tubes.</li>
	<li>To exclude Percoll, dilute the cell suspension with Locke&#39;s solution and centrifuge at 300 x g for 10 min at room temperature before re-suspending the pellet in Locke&#39;s solution. The estimated cell density of the isolated cell suspension is approximately 4 million cells/mL.</li>
	<li>For amperometric recording of exocytosis and intracellular cytometry measurements, plate chromaffin cells in collagen IV coated 60 mm plastic dishes at a density of about 17.5 &#215; 103 cells/cm2 and incubate the cells at 37 &#176;C in a 5% CO2 environment. Perform the electrochemical experiments within 1-3 days of cell culture.</li>
	<li>For the TEM imaging experiments, plate chromaffin cells in 75 cm2 cell culture flasks at a density of 7-8 million cells per flask and incubate at 37 &#176;C in a 5% CO2 environment for 1 day.</li>
</ol>
2. Single Cell Exocytosis Amperometry Experiments24
<ol>
	<li>To fabricate carbon fiber microelectrodes for these experiments, take a glass capillary with an outer diameter suitable for the electrode holder at the head stage that will be used in these experiments. Use a borosilicate glass capillary with an outer diameter of 1.2 mm and an inner diameter of 0.69 mm.
	<ol>
		<li>Connect one of the capillary ends to a water aspiration tube. Place 5 &#181;m diameter carbon fibers on something, such as a piece of white paper, to enhance visualization.</li>
		<li>Identify a single carbon fiber and hold the fiber down on one end with a finger to keep the carbon fiber in place while positioning the open end of the capillary in proximity to the free end of the carbon fiber. Gently aspirate the carbon fiber into the glass capillary so that the carbon fiber sticks out through both ends of the capillary. Move away the aspiration force.</li>
	</ol>
	</li>
	<li>Place the capillary with the carbon fiber into a micropipette puller and pull the glass capillary into two separate glass pipette tips. To disconnect the carbon fiber that is connected between the two glass tips, use a pair of scissors to cut the carbon fiber and gain two carbon fiber microelectrodes.</li>
	<li>Under a microscope, place the carbon fiber on top of a thicker microscope slide that allows manual cutting of the carbon fiber at the edge of where the fiber is extending from the glass capillary coating using a scalpel.</li>
	<li>After cutting the carbon fiber, leaving a glass coated carbon fiber tip, insert a few mm of the electrode tip into an Epoxy solution for 10 min to pull up epoxy and seal any possible open space between the carbon fiber and the surrounding glass. Lift the electrodes slowly out of the epoxy solution to prevent bulky glue drops from forming at the tip of the electrode.</li>
	<li>Place the electrodes on a holder (e.g., a wooden flat stick) with two-side sticky heat resistant tape to which electrodes can be attached. Bake the epoxy treated electrodes overnight in an oven at 100 &#176;C. The electrode tips easily break if they come into contact with a surface, so ensure the electrodes always are safely stored using a holder where the electrodes are fixed in place and tips do not risk being touched.</li>
	<li>To obtain a flat disc electrode surface, place the electrode in the holder of a microgrinder and bevel each carbon fiber electrode at an angel of 45&#176;. After beveling, mark the capillary on its topside using a permanent marker to later know how to locate the disc electrode surface at a 45&#176;&#160;angle when placing the electrode near cells for the exocytosis measurement. 
	NOTE: This step is important as in these experiments, the oval disc electrode needs to be placed flat on top of cells with its surface parallel to the surface of the Petri dish. Also, beveling electrodes are done the same day as experiments to ensure a fresh and clean electrode surface.</li>
	<li>Before use, place each carbon fiber microelectrode in a test solution (e.g., 0.1 mM dopamine in PBS buffer (pH 7.4)) to monitor the steady state current using cyclic voltammetry. For a cyclic voltammetry scan, apply a triangle potential waveform from -0.2 V to +0.8 V vs a Ag/AgCl reference electrode at 100 mV/s to ensure good reaction kinetics data are obtained that are in agreement with theoretically calculated values for a 5 &#181;m diameter disc carbon fiber microelectrode25.</li>
	<li>For amperometry recording of exocytosis, place the Petri dish with cultured chromaffin cells onto an inverted microscope. It is important to shield the microscope set up with a Faraday cage to eliminate electronic noise during the amperometry recording, due to the very small currents being measured. Use a microscope heating stage to maintain a temperature of 37 &#176;C during the cell experiments .</li>
	<li>Use a low-noise patch clamp instrument to apply a constant potential of +700 mV at the working electrode versus a Ag/AgCl reference electrode that is also placed in the Petri dish away from the working electrode. For recording exocytosis of chromaffin cells, digitalize the signal at 10 kHz and apply an internal low pass Bessel filter at 2 kHz to filter the recorded signal.</li>
	<li>To perform amperometric recording at single cells, mount the freshly beveled and tested carbon fiber disc microelectrode in the electrode holder of the head stage that is used with the potentiostat.
	<ol>
		<li>Gently place the electrode with the flat oval disc shape electrode surface facing down towards the apical surface of the cell and place the electrode in contact with the cell membrane using a micromanipulator.</li>
		<li>Adjust the distance from the electrode to the cell by monitoring the cell deformation caused by the electrode upon placement on top of the cell membrane and then carefully retract the electrode to a distance where the cell regains a shape close to its original cell shape. The ideal for kinetic and quantitative recording is to create a thin liquid film of a hundred nanometers to separate the electrode and cell surface, which are similar conditions for postsynaptic detection of chemical release in a synapse.</li>
	</ol>
	</li>
	<li>To stimulate the cells to exocytosis, position a glass micropipette with a tip size of 2-3 &#181;m diameter, filled with 5 mM BaCl2 solution at a distance of at least 20 &#181;m away from the cell, to prevent any solution leaking from the pipette tip to influence the experiment and apply a 5 s injection pulse of 5 mM BaCl2 solution at the cell surface to stimulate the cell to exocytosis.</li>
	<li>To study the reversible effects of osmotic pressure on the exocytosis process, prepare an isotonic buffer solution (150 mM NaCl, 5 mM KCl, 1.2 mM MgCl2, 5 mM glucose, 10 mM HEPES, pH 7.4) with 310 mOsm/kg iso-osmotic pressure and a hypertonic buffer made by adjusting the NaCl concentration of the isotonic buffer solution with an osmolality corresponding to 730 mOsm/kg.</li>
	<li>Place the cells in the isotonic buffer and stimulate the cell to exocytosis by applying a barium injection pulse while recording the amperometric current transients during the initiated exocytosis activity for approximately 3 min.
	<ol>
		<li>To compare the exocytosis responses in isotonic conditions to hypertonic conditions, incubate the cells for 10 min in hypertonic buffer solution and thereafter apply a barium injection pulse to stimulate exocytosis and perform 3 min of amperometric recording.</li>
		<li>For the reversible response of cells, incubate cells again for 10 min in isotonic buffer solution and stimulate cells by applying a 5s barium injection pulse and perform 3 min of recording the exocytosis response from the cell.</li>
	</ol>
	</li>
	<li>As control experiments to determine the effect on exocytosis activity by multiple barium stimulations, perform an amperometric recording of exocytosis release from three consecutive BaCl2 stimulations on the same cell placed in isotonic buffer and using the same time protocol for the consecutive cell incubation experiments with different osmolarity.</li>
</ol>
3. Intracellular Electrochemical Cytometry24,26
<ol>
	<li>To fabricate electrodes for vesicle quantal size measurements, use the same materials and start preparing a 5 &#181;m in diameter carbon fiber electrode according to the descriptions in sections 2.1 and 2.2 of microelectrode fabrication for amperometric exocytosis measurements.</li>
	<li>Under a microscope, use a scalpel to cut the carbon fiber extending out of the glass tip so that a carbon fiber with a length ranging from 30 to 100 &#181;m is left sticking out from the glass tip.</li>
	<li>To prepare a flame etched tip of the carbon fiber electrode, use a butane flame. To achieve an evenly etched, cylindrical shaped electrode tip, hold the cylindrical shaped carbon fiber electrode while rotating it and place the carbon fiber extending from the glass into the blue edge of the butane flame until the tip of the carbon develops a red color. This often takes less than 2 s. If successful, this results in an etched electrode tip size of 50-100 nm in diameter (a SEM image of such tip is shown in Figure 5B). After flame etching, place the electrode under a microscope to evaluate the electrode tip.</li>
	<li>Insert the cylindrical nanotip microelectrode in epoxy solution for 3 min followed by a 15 s dipping of the electrode tip into an acetone solution. This allows epoxy to seal the potential gap space between the carbon fiber and the insulating glass capillary wall, while the acetone clears the epoxy off the etched carbon fiber electrode surface. To cure the epoxy, bake the electrodes in an oven overnight at 100 &#176;C.</li>
	<li>Before use, test the steady state current of each carbon fiber microelectrode, as explained in section 2.7 using cyclic voltammetry. For experiments, only use electrodes that display a plateau current around 1.5-2.5 nA27.</li>
	<li>For intercellular amperometry measurements, place the cells at the microscope as described in 2.8 and use the same experimental settings of the potentiostat as described in 2.9.</li>
	<li>To perform intracellular amperometric measurement, and to prevent significant physical damage to the cell, insert the nanotip cylindrical microelectrode into the cell by adding a gentle mechanical force, just enough to push the electrode through the cell plasma membrane and into the cell cytoplasm using a micromanipulator.</li>
	<li>After insertion, and with the cell membrane sealed around the cylindrical electrode, start the amperometric recording in situ at the live cell. At the oxidation potential that is applied to the electrode, vesicles will adsorb to the electrode surface and stochastically rupture.&#160; Hence, there is no need for any kind of stimulus to initiate this process.</li>
	<li>To determine the osmotic effect on vesicle quantal size, collect the intracellular cytometry measurements from a group of cells that have been incubated in isotonic and in hypertonic buffer using the experimental condition as described in section 2.13.</li>
</ol>
4. Data Analysis of Amperometry Recordings
<ol>
	<li>To analyze the recorded amperometry data from exocytosis and intracellular vesicle quantal size analysis, use a software program that allows analysis of current transients in the recorded current versus time trace so that kinetic peak parameters and the integrated total charge for individual current peaks can be determined. For data analysis, we have used software developed in the Sulzer lab that was written for the data analysis program Igor28.</li>
	<li>When analyzing the amperometric spikes, select a threshold limit for peaks of three times the root-mean square (RMS) standard deviation of the noise for each recording.</li>
	<li>Collect the amperometric spikes from each cell recording manually to prevent false spikes that do not follow the Gaussian shape, double spikes which can be the result of merged exocytosis events, and only accept Gaussian shaped spikes with a threshold of three times higher than the RMS noise.</li>
	<li>Collect the data for total charge per single amperometric peak and use Faradays law (N=QnF) to calculate the molar amount of catecholamine neurotransmitter detected per exocytosis or intracellular single vesicle rupture event, where N is the moles of neurotransmitters going through a redox reaction at the electrode surface, Q=the total charge detected under each spike, n=number of electrons transferred in the redox reaction (n=2 for catecholamines), and the Faraday&#180;s constant F=96485 C/mol.</li>
	<li>Perform statistical analysis of the data collected by first calculating the average charge detected per event for each cell. Then for variance between cells, calculate the average charge between cells and use a student&#39;s t-test between cells assuming unequal variance. This study used the MATLAB program for statistical analysis.</li>
</ol>
5. TEM Imaging for Vesicle Size Analysis
<ol>
	<li>To perform TEM imaging of cells at the different osmotic conditions, first incubate the cells in isotonic or hypertonic buffer for 10 min at 37 &#176;C in a 5% CO2 environment before chemical fixation of cells.</li>
	<li>Perform cell fixation using the Karnovsky fixative method29. Using this method, incubate the cells with a solution containing 0.01% sodium azide, 1% formaldehyde, and 1.25% glutaraldehyde in which the sample can be stored at 4 &#176;C.</li>
	<li>After fixation, wash the cells with 0.15 M sodium cacodylate buffer.</li>
	<li>To stain the cell samples post fixation, and in preparation for TEM imaging, incubate the cells with a 1% osmium tetroxide solution for 2 h at 4 &#176;C, followed by 1 h incubation in 0.5% uranyl acetate solution at room temperature in the dark.</li>
	<li>In a final fixation step, dehydrate the cells first by rinsing the cells in 100% ethanol and then rinse cells with acetone.</li>
	<li>Embed the cell samples in epoxyresin and thereafter perform centrifugation at 4,000 x g for 30-40 min and allow the cell sample to polymerize at 40 &#176;C for 15 h followed by 48 h incubation at 60 &#176;C.</li>
	<li>In preparation for imaging, section the cell sample embedded in Agar 100 resin into slices with thickness of 60 nm using an ultramicrotome.</li>
	<li>Subject the cells to a 4% uranyl acetate/25% ethanol solution for 4 min followed by 20 s of rinsing with water. Wash the cells with Reynolds lead citrate for 3 min, followed by 20 s of rinsing with water.</li>
	<li>Perform transmission electron microscopy imaging of cell samples. In our experiments, we have used a transmission electron microscope that has been operated at 120 kV.</li>
	<li>From each recorded image of a cell section illustrating the cell ultrastructure that displays a population of the vesicles in the cell cytoplasm, first calibrate the image pixel size by relating pixels to the recorded scale bar in each TEM image. Use imaging software to determine the vesicle sizes at each image of cells exposed to isotonic or hypertonic conditions. In our experiments, we used the software ImageJ for image analysis. It is worth noting that for image analysis of cellular ultrastructure from TEM images of cells, size adjustment of these measurements based on thickness of cell sections needs to be considered and have been previously described by Almers&#180;s lab30.</li>
</ol>

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<li>Mosharov, E. V., Sulzer, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Analysis+of+exocytotic+events+recorded+by+amperometry%5BTitle%5D)+AND+%22Nat+Methods%22%5BJournal%5D)">Analysis of exocytotic events recorded by amperometry.</a> Nat Methods. 2 (9), 651-658 (2005).</li>
<li>Morris, J. K. <a target="_blank" href="https://www.researchgate.net/publication/244955881_A_Formaldehyde-Glutaraldehyde_Fixative_of_High_Osmolality_for_Use_in_Electron_Microscopy">A formaldehyde glutaraldehyde fixative of high osmolality for use in electron microscopy.</a> J Cell Biol. 27, 137-139 (1965).</li>
<li>Parsons, T. D., Coorssen, J., Horstmann, H., Almers, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Docked+granules%2C+the+exocytic+burst%2C+and+the+need+for+ATP+hydrolysis+in+endocrine+cells%5BTitle%5D)+AND+%22Neuron%22%5BJournal%5D)">Docked granules, the exocytic burst, and the need for ATP hydrolysis in endocrine cells.</a> Neuron. 15 (5), 1085-1096 (1995).</li>
</ol>

The authors have nothing to disclose.

We here present a protocol and the advantages of combining three complementary analytical methods to analyze secretory vesicles and the exocytosis process to gain a better understanding of how a physical force such as osmotic pressure can affect secretory vesicles and the exocytosis process in secretory cells. These methods include carbon fiber microelectrode amperometry, which is an established method for recording exocytosis activity, intracellular electrochemical cytometry, which is used to determine quantal size of vesicles in their native environment, and transmission electron microscopy image analysis to monitor secretory vesicle volume. In this work, by collecting quantitative data from amperometry recordings of single vesicle exocytosis events at chromaffin cells exposed to an isotonic and a hypertonic extracellular environment, we confirmed that osmotic shock significantly reduces the amount neurotransmitters released during exocytosis and that these cells can reversibly recover and release the original quantity, if placed back into an isotonic environment (Figure 3).
The amperometric recordings provided information of the frequency of exocytosis events versus time and therefore can also be used to monitor changes in exocytosis activity at cells in different osmotic environments. This data can be interpreted and used to discern whether alterations in activity occur instantly or as a function of time. As we showed in previous work, although osmotic stress hampered exocytotic activity, it did not seem to hinder the fusion of the readily releasable pool of vesicles24. The exocytosis activity data can also be used to analyze the total exocytotic activity during a period of recording time. Here we present the accumulated number of exocytosis events from a 3-minute recording of exocytosis at chromaffin cells exposed to the two different osmotic conditions. These data show an inhibition in exocytosis activity of cells experiencing osmotic stress and that a partial recovery of this activity can be achieved after cells return to an extracellular isotonic environment. However, very importantly, the control experiments showed that multiple Ba2+ stimulations within the time frame used in these experiments caused a significant reduction in exocytosis activity by each time a cell was stimulated to secretion. By the third consecutive Ba2+ stimulation, only a third of the exocytosis activity was maintained, and clearly the barium, and perhaps also the timing of stimulations in these experiments, was affecting the vesicle cycle. This might be relevant for explaining why exocytotic activity was recovered in cells placed in isotonic solution after the osmotic shock and why these cells displayed a similar relative reduction in activity compared with cells in isotonic conditions after three sequential Ba2+ stimulations. Hence, amperometry recording of exocytosis provides information on secretory vesicles from the moment the vesicles are triggered to fuse with the plasma membrane, releasing neurotransmitters through the fusion pore. Thereby quantitative data on single vesicle neurotransmitter release and information on the exocytosis activity can be collected.
The quantity of neurotransmitter released can be regulated by the mode of exocytosis that is triggered, where either the full vesicle content or part of the content is released. By solely studying exocytosis release using carbon fiber amperometry that only detects what is expelled from a vesicle, it is difficult to distinguish if a change in the detected amount of neurotransmitter released is related to an alteration in the triggered mode of exocytosis, a change in the cellular biophysical properties affecting vesicle content release, or to changes in vesicle quantal size. Therefore, by complementing the amperometric recording of exocytosis with measurements using the intracellular electrochemical cytometry, in situ measurements of vesicle quantal size at live cells can be characterized and hence used to compare the fraction of vesicle content release from vesicles during exocytosis26.
In this work, to investigate if the vesicle quantal size was affected by osmotic stress, we applied this technique for the quantification and evaluation of vesicle quantal size at cells exposed to isotonic and hypertonic conditions. As insertion of the nanotip electrode into the cytoplasm of a live cell is considered rather invasive, these experiments were only performed once per cell and were not repeated at the same cell. Therefore, these experiments are preferentially performed as individual measurements from groups of randomly selected cells exposed to an isotonic and a hypertonic extracellular environment. To compare changes in vesicle quantal size as measured by intracellular electrochemical cytometry to alterations in the amount neurotransmitter released at exocytosis, one should consider matching the experimental conditions of intracellular recording and also perform amperometry recording of exocytosis at separate random cells. If studies are performed on the same single cell, it is important in these experimental protocols to also consider the influence of consecutive BaCl2 stimulations, and to ensure the experimental conditions match those used for intracellular cytometry measurements. It is also worth noting that it is difficult to control the exact placement and depth of the electrode when is inserted into a cell. Thus, each cell provides a random sample for vesicle quantal size analysis. In addition, probing vesicle quantal size using this method does not distinguish differences in, for instance, vesicle maturity and therefore also might add variation to measurements. Intracellular experiments showed that vesicle quantal size was reduced at cells exposed to extracellular osmotic pressure. The relative reduction in quantal size detected by this method was compared to the observations of relative changes in neurotransmitter release during exocytosis. This study found that the relative decline in quantal size was on the same order as the drop in neurotransmitter release at cells sensing osmotic stress.
To verify if osmotic stress was altering the vesicle neurotransmitter concentration, the vesicle volume was evaluated using TEM imaging analysis for chemically fixed chromaffin cells that had been exposed to isotonic and hypertonic conditions. TEM imaging analysis showed that vesicles shrink when cells are exposed to an osmotic shock and that the relative reduction in size is adjusted together with the vesicle quantal size to maintain a constant neurotransmitter concentration24. The TEM image analysis, which provides nanometer image resolution can distinguish the two phases, the dense core protein matrix and the surrounding halo solution inside LDCVs, and thus makes it possible to determine the volume of dense core protein matrix and calculate the volume of the halo solution. From this analysis, the decline in vesicle volume was determined to be mainly related to a diminishing volume from the halo solution surrounding the dense core protein matrix24.
In summary, this study presents a protocol demonstrating how three analytical methods is combined, and allows characterization of secretory vesicles before neurotransmitter release and what are released from these vesicles when cells are triggered to exocytosis, to gain a better understanding of how secretory vesicles and cell functions like exocytosis is affected by extracellular stress. This protocol might also be used to help answer questions on how neurotransmitter release at exocytosis and vesicle quantal size is affected by other alterations in the physical environment or by potential drugs that may affect secretory cells.

Chromaffin cells in adrenal glands are neuroendocrine cells that release neurotransmitter molecules into the blood stream. This occurs through a cellular process that involves the docking and fusion of neurotransmitter-filled vesicles, resulting in content release from vesicles to the extracellular space in a process called exocytosis. The neurotransmitters (adrenaline and noradrenaline) in chromaffin cells are actively transported by membrane proteins into large dense core vesicles (LDCVs) and stored at high concentrations (~0.5-1 M)1,2. Accumulation of neurotransmitters inside the LDCVs is accomplished by the affinity of catecholamine molecules to the intravesicular dense core protein matrix comprised of chromogranin proteins (~169 mg/mL)3,4,5,6, and an intravesicular cocktail solution containing key components for catecholamine loading and storage into the vesicle such as ATP (125-300 mM)7, Ca2+ (50-100 &#181;M in the solution and ~40 mM bound to the protein matrix)8, Mg2+ (5 mM)9, ascorbate (10-30 mM)10, and a pH of ~5.511,12. The LDCVs maintain an iso-osmotic condition with the cell cytoplasm (310 mOsm/kg)13, even though the theoretical solute concentration inside the vesicles sum up to more than 750 mM. The composition of the intravesicular components is not only essential for the loading and storage of catecholamines, but also for aggregation of solutes to the dense core protein matrix. This significantly reduces the osmolarity of the vesicles is significantly reduced and can affect the amount catecholamine that is released during exocytosis5,6.
Studies on the effect of extracellular osmotic pressure on the exocytosis process by amperometric recording have reported that high extracellular osmotic pressure inhibits exocytosis activity and reduces the number of neurotransmitters secreted from single vesicle compartments4,14,15,16,17,18,19. The explanations of these observations have speculated on the possible enhancement of macromolecular crowding in the cell cytoplasm inhibiting vesicle fusion events, and an alteration in membrane biophysical properties affecting the number of neurotransmitters released during exocytosis. These thoughts assumed that high extracellular osmotic stress does not affect the vesicle quantal size, which defines the number of neurotransmitter molecules stored in a vesicle compartment at prior stage of triggered exocytosis14,15,17,19,20,21. In amperometric measurements of exocytosis release in single cells, a carbon fiber disc microelectrode is placed in close contact with the cell surface, creating an experimental set up mimicking the synapse configuration, where the amperometric electrode serves as a postsynaptic detector (Figure 1)22,23. By stimulating a cell to exocytosis, one can induce neurotransmitter-filled vesicles to fuse with the cell plasma membrane and release part or the full vesicle content into the extracellular space. These neurotransmitter molecules released at the surface of the electrode can be detected electrochemically if the neurotransmitters are electroactive (e.g., catecholamines) by applying a redox potential of +700 mV vs a Ag/AgCl reference electrode. Consequently, a series of current spikes mark the detection of individual exocytosis events. From the current versus time trace in an amperometric recording, the area under each single amperometric spike represents the charge detected per exocytosis event and can be converted to the mole of neurotransmitters released, using the Faraday equation. Hence, the amperometric recordings provide quantitative information on the amount neurotransmitters expelled from single exocytosis events and report on the frequency of exocytosis events, but do not present quantitative information on the secretory vesicles content before vesicle fusion and neurotransmitter release has been initiated.
Therefore, to get a better understanding of how secretory vesicles in the cell cytoplasm respond to extracellular osmotic stress before the cell is triggered to undergo exocytosis, other complementary analytical methods can be used to enrich this information. For instance, to investigate if osmotic stress alters vesicle volume, transmission electron microscopy (TEM) imaging analysis can be used to measure the vesicle size of cells after chemical fixation. To examine if osmotic stress affects vesicle quantal size, a recently developed amperometric technique called intracellular electrochemical cytometry, can be applied for quantification of vesicle neurotransmitter content at secretory vesicles in their native state when still residing in the cytoplasm of live cells26. In the intracellular electrochemical cytometry technique, a nanotip cylindrical carbon fiber electrode is gently inserted into the cytoplasm of live cells and, by applying a +700 mV potential to this electrode (vs a Ag/AgCl reference electrode), the catecholamine content in vesicles can be quantified by the detection of a redox current spike from single vesicles colliding, adsorbing, and subsequently stochastically rupturing at the electrode surface and thereby releasing their contents against the electrode surface26. Hence, in the amperometric current versus time trace, each single vesicle rupturing event can result in a current transient and, by integrating the area of each current spike, the vesicle quantal size can be calculated using Faraday&#180;s law.
Therefore, by linking the quantitative information gained from vesicle size measurements using TEM imaging together with vesicle quantal size analysis, as recorded by intracellular electrochemical cytometry, vesicle neurotransmitter concentration can also be determined. This allows vesicle characterization when cells are exposed to different osmotic conditions and provides a better view on how vesicles may respond to extracellular osmotic stress at the stage prior to exocytosis. The results from combining these methods have shown that in the presence of extracellular high osmotic pressure, vesicles shrink and adjust their quantal size and comparing the quantitative information on the relative changes from these measurements shows that while shrinking, vesicles adjust their contents and size to maintain a constant neurotransmitter concentration24. Thus, this understanding is valuable in connecting to the observations made on neurotransmitter release in cells exposed to osmotic stress. In these protocols, we describe the use of these three complementary methodologies that allow the characterization of how secretory vesicles in their native environment respond to extracellular osmolality and the effects of this response on the exocytosis process. In addition to our previous observations regarding the effect of high osmotic pressure on exocytosis24, we present additional experiments that describe cell recovery after osmotic shock and the effect of multiple barium stimulations in chromaffin cells.

<table><tbody><tr><td>NaCl</td><td>Sigma Aldrich</td><td>S7653</td><td></td></tr><tr><td>KCl</td><td>Sigma Aldrich</td><td>P9333</td><td></td></tr><tr><td>NaHCO&lt;sub&gt;3&lt;/sub&gt;</td><td>Sigma Aldrich</td><td>S5761</td><td></td></tr><tr><td>HEPES</td><td>Sigma Aldrich</td><td>H3375</td><td></td></tr><tr><td>MgCl2</td><td>Sigma Aldrich</td><td>M-2670</td><td></td></tr><tr><td>Glucose</td><td>Sigma Aldrich</td><td>G8270</td><td></td></tr><tr><td>Collagenase P</td><td>Roche, Sweden</td><td>11 213 857 001</td><td></td></tr><tr><td>100-&amp;micro;M Nylon mesh</td><td>Fisher Sientific</td><td>08-771-19</td><td></td></tr><tr><td>Percoll</td><td>Sigma Aldrich</td><td>P1677</td><td></td></tr><tr><td>Collagen IV coated 60 mm plastic dish</td><td>VWR</td><td>354416</td><td></td></tr><tr><td>Centrifuge</td><td>Avanti J-20XP</td><td></td><td></td></tr><tr><td>Borosilicate glass capillary</td><td>Sutter instrument Co., Novato, CA</td><td></td><td></td></tr><tr><td>Micropipette puller</td><td>Narishing Inc., Japan</td><td>PE-21</td><td></td></tr><tr><td>Epoxy solutions (A and B)</td><td>Epoxy technology, Billerica, MA</td><td></td><td></td></tr><tr><td>Beveller</td><td>Narishing Inc.</td><td>EG-400</td><td></td></tr><tr><td>Inverted Microscope</td><td>Olympus</td><td>IX81</td><td></td></tr><tr><td>Patch clamp Instrument</td><td>Molecular Devices, Sunnyvale, CA</td><td>Axopatch 200B</td><td></td></tr><tr><td>Micromanipulator</td><td>Burleigh Instrument Inc., USA</td><td>PCS-5000</td><td></td></tr><tr><td>Butane Flame</td><td>Multiflame AB, H&amp;auml;sselholm, Sweden</td><td></td><td></td></tr><tr><td>Transmission electron microscopy</td><td>Omega</td><td>Leo 912 AB</td><td></td></tr></tbody></table>

monitoring the effect of osmotic stress on secretory vesicles and exocytosis

Amperometry recording of cells subjected to osmotic shock show that secretory cells respond to this physical stress by reducing the exocytosis activity and the amount of neurotransmitter released from vesicles in single exocytosis events. It has been suggested that the reduction in neurotransmitters expelled is due to alterations in membrane biophysical properties when cells shrink in response to osmotic stress and with assumptions made that secretory vesicles in the cell cytoplasm are not affected by extracellular osmotic stress. Amperometry recording of exocytosis monitors what is released from cells the moment a vesicle fuses with the plasma membrane, but does not provide information on the vesicle content before the vesicle fusion is triggered. Therefore, by combining amperometry recording with other complementary analytical methods that are capable of characterizing the secretory vesicles before exocytosis at cells is triggered offers a broader overview for examining how secretory vesicles and the exocytosis process are affected by osmotic shock. We here describe how complementing amperometry recording with intracellular electrochemical cytometry and transmission electron microscopy (TEM) imaging can be used to characterize alterations in secretory vesicles size and neurotransmitter content at chromaffin cells in relation to exocytosis activity before and after exposure to osmotic stress. By linking the quantitative information gained from experiments using all three analytical methods, conclusions were previously made that secretory vesicles respond to extracellular osmotic stress by shrinking in size and reducing the vesicle quantal size to maintain a constant vesicle neurotransmitter concentration. Hence, this gives some clarification regarding why vesicles, in response to osmotic stress, reduce the amount neurotransmitters released during exocytosis release. The amperometric recordings here indicate this is a reversible process and that vesicle after osmotic shock are refilled with neurotransmitters when placed cells are reverted into an isotonic environment.

We here describe the protocol for how combining TEM imaging together with two electrochemical methodologies, carbon fiber amperometry and intracellular electrochemical cytometry, can provide information that gains a broader view alluding to the effect of extracellular osmotic pressure on secretory vesicles and the exocytosis process. By comparing representative amperometric recordings of exocytosis release at single chromaffin cells using the experimental set up (shown in Figure 1), a significant reduction in exocytotic activity was displayed when cells were exposed to osmotic stress as compared to cells in isotonic conditions (Figure 2A)24. From these recordings and by using Faraday&#180;s law, the total charge detected by each individual amperometric current spike was used to calculate the number of molecules expelled from single vesicle exocytosis events at cells exposed to the different osmotic conditions. By comparison, as displayed in Figure 2B by the smaller area of the average amperometric current spike detected by cells in hypertonic solution, fewer neurotransmitter molecules were released from each vesicle by cells sensing osmotic stress24.
To determine the reversibility of this decline in the number of neurotransmitter molecules released, we performed amperometric recordings of exocytosis at cells exposed to a hypertonic environment and, subsequently, at cells after placed back into an isotonic environment. In these experiments, chromaffin cells were stimulated three consecutive times with BaCl2 solution: first in an isotonic buffer, followed by a second stimulation after cells were incubated for 10 min in a hypertonic solution and, finally, a third stimulation after 10 min cell incubation in isotonic conditions. The results as displayed in Figure 3A present that the quantity of neurotransmitters released was reduced by ~50% when cells were exposed to the hypertonic condition compared to the first Ba2+ stimulation in the isotonic condition. Subsequently, when cells were brought back to an isotonic environment and subjected to a third Ba2+ stimulation, the amount neurotransmitter released per exocytosis event was reversed back to the original amount recorded at the first stimulation, which confirmed previous observations14. Control experiments with three successive Ba2+ stimulations of cells in the isotonic condition (see Figure 3B) show that multiple sequential Ba2+ stimulations in isotonic conditions did not alter the amount neurotransmitter released during exocytosis. This suggests that vesicle quantal size is quickly and reversibly adjusted with extracellular osmolarity.
However, when analyzing the amperometric traces from these experiments in terms of exocytosis activity, it became evident, as displayed in Figure 4A, that exocytosis activity was significantly hampered when cells were exposed to hypertonic stress. During osmotic stress, exocytosis events were reduced to 12% of the activity at cells in isotonic condition. Subsequently, after the osmotic shock and cells were placed back into an isosmotic environment, cells regained 41% of their original exocytosis activity. Interestingly, the control experiments performed in isotonic conditions showed, as displayed in Figure 4B, that after performing three consecutive BaCl2 stimulations, the frequency of exocytosis events was reduced to 53% after a second stimulation and further down to 26% by the third stimulation compared to the first stimulation. Hence, it is clear that consecutive Ba2+ stimulations do not seem to affect the number of neurotransmitters released from each vesicle when exocytosis is triggered, but is significantly influencing the efficiency of the vesicle release process.
To investigate how secretory vesicles in their native environment are affected by extracellular osmotic stress in terms of vesicle volume or quantal size, vesicle size analysis using TEM imaging was combined with intracellular electrochemical cytometry at cells exposed to isotonic and hypertonic conditions. In the intracellular electrochemical cytometry experiments, a carbon fiber nanotip electrode was inserted into the cytoplasm of live chromaffin cells when placed in isotonic and hypertonic solution (as shown in Figure 5.) The resulting amperometric current spike was monitored of each vesicle in the cell cytoplasm colliding, adsorbing, and stochastically rupturing and releasing the vesicle contents at the surface of the amperometric electrode upon bursting26. The integrated total charge detected for each peak in the current versus time trace was used to calculate the average vesicle quantal size in each cell recording by Faraday&#180;s law. These intracellular electrochemical cytometry measurements, shown in Figure 6 and Figure 7B, demonstrated that vesicle quantal size at cells exposed to osmotic stress were significantly reduced compared to at cells in isotonic conditions. Comparing the magnitude of alteration in vesicle quantal size as measured by intracellular electrochemical cytometry, to the fractional decline in the quantity of neurotransmitter released during exocytosis at cells experiencing extracellular osmotic stress, showed a relative decrease of 60% in both quantal size and the amount neurotransmitter released compared to at cells in isotonic conditions (Figure 7)24. To relate the adjustment in vesicle quantal size to a potential variation in vesicle neurotransmitter concentration of cells experiencing osmotic pressure, TEM image analysis was performed to determine the vesicle size of cells exposed to isotonic and hypertonic conditions. Furthermore, the dark staining of the dense core protein matrix inside the LDCVs that is visualized in the TEM images as a dark sphere in the membrane bound vesicles was used to measure the volume of dense core matrix in these vesicles. As presented in Figure 8, vesicle size was reduced to 60% at cells exposed to extracellular osmotic stress compared to at cells in isotonic conditions. From the calculated volume of the measured diameter of the LDCV and the dense core, the volume of the surrounding halo solution that appears as a clear solution inside the LDCVs in the TEM images was also calculated. The summarized results from the TEM image analysis showed, as displayed in Figure 8, that during extracellular osmotic shock it is mainly the volume of the halo solution in the LDCVs that is reduced24.

<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/56537/56537fig1.jpg" /> 
Figure 1: Single cell exocytosis amperometry. A schematic of the experimental set up for amperometric measurement of exocytosis at single chromaffin cells24. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/56537/56537fig2.jpg" /> 
Figure 2: Amperometric traces from exocytosis measurements.&#160;(A) A representative amperometric recording of exocytosis at chromaffin cells in isotonic (black color) and in hypertonic (red color) extracellular environments. (B) Enlargement of an average amperometric spike from exocytosis measurement of chromaffin cells in isotonic (black) and hypertonic (red) extracellular environments24. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/56537/56537fig3.jpg" /> 
Figure 3: The reversibility of the number of catecholamines released at exocytosis after osmotic shock. (A) The number of molecules released during exocytosis from chromaffin cells (n=4) by three consecutive Ba2+ stimulations, with the first stimulation in isotonic, the second in hypertonic, and the third in isotonic buffer. The statistical results of the unpaired t-test are shown. The p-value for comparison of the first Ba2+ stimulation (Ba2+ stim 1) in isotonic buffer with the second Ba2+ stimulation (Ba2+ stim 2) in hypertonic buffer is p=0.1088 and the p-value for the comparison of the second Ba2+ stimulation in hypertonic solution with the third Ba2+ stimulation (Ba2+ stim 3) in isotonic buffer is p=0.059. (B) Control experiment demonstrating the amount of neurotransmitter molecules released at three consecutive Ba2+ stimulations of chromaffin cells (n= 4) in isotonic buffer. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/56537/56537fig4.jpg" /> 
Figure 4: The effect of osmotic pressure on exocytosis activity. (A) The effect of extracellular osmolarity on exocytosis activity is presented as the frequency of exocytosis events when chromaffin cells (n= 4) are stimulated with barium solution in isotonic, then hypertonic, and finally in isotonic conditions. The values are presented as the average number of spikes from each cell and the average from all cells sampled ( standard error of the mean (SEM)). The statistical significance of changes is presented using a t-test for unpaired data (the p-value for isotonic Ba2+ stimulation 1 and hypertonic Ba2+ stimulation 2 is p=0.0126 and the p-value for comparison of hypertonic Ba2+ stimulation 2 and isotonic Ba2+ stimulation 3 is p=0.037).(B) Control experiment presenting the frequency of exocytosis events after three consecutive barium stimulations at chromaffin cells (n=4) in isotonic conditions. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/56537/56537fig5.jpg" /> 
Figure 5: Intracellular vesicle electrochemical cytometry to monitor changes in vesicle quantal size. (A) A schematic of the experimental set up used for intracellular electrochemical cytometry. (B) A scanning electron microscopy image of a typical nanotip conical carbon fiber electrode24. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/56537/56537fig6.jpg" /> 
Figure 6: Intracellular electrochemical cytometry measurements showing (A) Representative traces of intracellular amperometric cytometry recordings at chromaffin cells in isotonic (black) and hypertonic (red) extracellular environments. (B) Enlargement of an average amperometric spike from intracellular cytometry measurement at chromaffin cells in isotonic (black) and hypertonic (red) extracellular environments24. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/56537/56537fig7.jpg" /> 
Figure 7: Quantification of the number of catecholamines released at exocytosis and determination of vesicle quantal size. (A) The average number of molecules released during exocytosis recordings at chromaffin cells in isotonic (n=22) and hypertonic (n= 20) environments. The values are presented as an average number of molecules released per exocytosis event from each cell and averaged from the cells sampled ( &#177; SEM). The statistical significance of changes are presented using t-test for unpaired data (p-value=0.0003) (B) The average number of molecules per vesicle as detected by intracellular electrochemical cytometry at chromaffin cells in isotonic (n=19) and hypertonic (n=16) conditions. The values are presented as the average number of molecules per spike as detected from each cell and averaged from all cells sampled ( &#177;&#160;SEM). The statistical significance of changes is presented using t-test for unpaired data (p- value=0.0108)24. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 8" class="xfigimg" src="/files/ftp_upload/56537/56537fig8.jpg" /> 
Figure 8: Effect of osmotic pressure on large dense core vesicle size. The calculated volume of the LDCVs, the dense core protein and the halo solution surrounding the dense core protein matrix was calculated in attolitres (aL) from image analysis of TEM images of chromaffin cells in isotonic (n=12) and hypertonic (n=9) buffers. The results were collected from an average of 311 vesicles per cell and averages from single cells ( &#177;&#160;SEM). The p-values are reported from unpaired t-tests comparing isotonic and hypertonic buffers. The P-value is 0.0385 (*) for vesicle volume, 0.3967 for dense core volume, 0.0047 (**) for halo volume24.&#160;<a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56537/56537fig8large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Monitoring the Effect of Osmotic Stress on Secretory Vesicles and Exocytosis at JoVE.com

Monitoring the Effect of Osmotic Stress on Secretory Vesicles and Exocytosis

Osmotic stress affects exocytosis and the amount of neurotransmitter released during this process. We demonstrate how combining electrochemical methods together with transmission electron microscopy can be used to study the effect of extracellular osmotic pressure on exocytosis activity, vesicle quantal size, and the amount of neurotransmitter released during exocytosis.

Amperometry recording of cells subjected to osmotic shock show that secretory cells respond to this physical stress by reducing the exocytosis activity ...

monitoring-effect-osmotic-stress-on-secretory-vesicles

Nanyang Technological University

Research

JoVE Journal

Neuroscience

8.5K Views.  Chalmers University of Technology. Osmotische stress beïnvloedt exocytose en de hoeveelheid neurotransmitter uitgebracht tijdens dit proces. We laten zien hoe elektrochemische methoden samen met transmissie-elektronenmicroscopie combineren kan worden gebruikt voor het bestuderen van het effect van extracellulaire osmotische druk op exocytose activiteit, blaasje quantal grootte en de hoeveelheid neurotransmitter vrijgegeven tijdens exocytose.

Video: Monitoring the Effect of Osmotic Stress on Secretory Vesicles and Exocytosis

Membrane Remodeling of Giant Vesicles in Response to Localized Calcium Ion Gradients

In a wide variety of fundamental cell processes, such as membrane trafficking and apoptosis, cell membrane shape transitions occur concurrently with local variations in calcium ion concentration. The main molecular components involved in these processes have been identified; however, the specific interplay between calcium ion gradients and the lipids within the cell membrane is far less known, mainly due to the complex nature of biological cells and the difficultly of observation schemes. To bridge this gap, a synthetic approach is successfully implemented to reveal the localized effect of calcium ions on cell membrane mimics. Establishing a mimic to resemble the conditions within a cell is a severalfold problem. First, an adequate biomimetic model with appropriate dimensions and membrane composition is required to capture the physical properties of cells. Second, a micromanipulation setup is needed to deliver a small amount of calcium ions to a particular membrane location. Finally, an observation scheme is required to detect and record the response of the lipid membrane to the external stimulation. This article offers a detailed biomimetic approach for studying the calcium ion-membrane interaction, where a lipid vesicle system, consisting of a giant unilamellar vesicle (GUV) connected to a multilamellar vesicle (MLV), is exposed to a localized calcium gradient formed using a microinjection system. The dynamics of the ionic influence on the membrane were observed using fluorescence microscopy and recorded at video frame rates. As a result of the membrane stimulation, highly curved membrane tubular protrusions (MTPs) formed inside the GUV, oriented away from the membrane. The described approach induces the remodeling of the lipid membrane and MTP production in an entirely contactless and controlled manner. This approach introduces a means to address the details of calcium ion-membrane interactions, providing new avenues to study the mechanisms of cell membrane reshaping.

We present a technique for contactless micromanipulation of vesicles, using localized calcium ion gradients. Microinjection of a calcium ion solution, in the vicinity of a giant lipid vesicle, is utilized to remodel the lipid membrane, resulting in the production of membrane tubular protrusions.

In a wide variety of fundamental cell processes, such as membrane trafficking and apoptosis, cell membrane shape transitions occur concurrently with local ...

Chemistry

Investigating Mast Cell Secretory Granules; from Biosynthesis to Exocytosis

Mast Cells (MC) are secretory cells of the immune system that accomplish their physiological and pathological functions by releasing pre-formed and newly synthesized allergic, inflammatory and immunoregulatory mediators. MCs&#8217; mediators affect multiple tissues and organs culminating in allergic and immune responses. The synthesis, storage and release of the MC mediators are highly regulated. The pre-formed mediators are packed in cytoplasmic secretory granules&#160;(SG) that fuse with the plasma membrane and release their content by regulated exocytosis. We present a protocol, based on the co-expression of a gene of interest with a reporter gene that is targeted to the SGs and is released in a regulated fashion alongside the endogenous SG mediators. The protocol enables high resolution four dimensional confocal analyses of the MC SGs and monitoring their timeline from biogenesis to triggered exocytosis. Thus, using this protocol for screening genes of interest for their phenotypic and functional impact allows deciphering the molecular mechanisms that govern the biogenesis and exocytosis of the MC SGs and identifying the regulators involved. Thereby, further insights into the cellular mechanisms that account for MCs function in health and disease should be provided.

The goal of the present&#160;protocol was to develop a method that will allow functional genomic analyses of mast cell secretion. The protocol is based on quantitative assessment of the release of a fluorescent reporter gene cotrasfected with the gene of interest and real time&#160;analyses of the secretory granule&#39;s morphology.

Mast Cells (MC) are secretory cells of the immune system that accomplish their physiological and pathological functions by releasing pre-formed and newly ...

Immunology and Infection

TIRFM and pH-sensitive GFP-probes to Evaluate Neurotransmitter Vesicle Dynamics in SH-SY5Y Neuroblastoma Cells: Cell Imaging and Data Analysis

Synaptic vesicles release neurotransmitters at chemical synapses through a dynamic cycle of fusion and retrieval. Monitoring synaptic activity in real time and dissecting the different steps of exo-endocytosis at the single-vesicle level are crucial for understanding synaptic functions in health and disease.
Genetically-encoded pH-sensitive probes directly targeted to synaptic vesicles and Total Internal Reflection Fluorescence Microscopy (TIRFM) provide the spatio-temporal resolution necessary to follow vesicle dynamics. The evanescent field generated by total internal reflection can only excite fluorophores placed in a thin layer (&#60;150 nm) above the glass cover on which cells adhere, exactly where the processes of exo-endocytosis take place. The resulting high-contrast images are ideally suited for vesicles tracking and quantitative analysis of fusion events.
In this protocol, SH-SY5Y human neuroblastoma cells are proposed as a valuable model for studying neurotransmitter release at the single-vesicle level by TIRFM, because of their flat surface and the presence of dispersed vesicles. The methods for growing SH-SY5Y as adherent cells and for transfecting them with synapto-pHluorin are provided, as well as the technique&#160;to perform TIRFM and imaging. Finally, a strategy aiming to select, count, and analyze fusion events at whole-cell and single-vesicle levels is presented.
To validate the imaging procedure and data analysis approach, the dynamics of pHluorin-tagged vesicles are&#160;analyzed under resting and stimulated (depolarizing potassium concentrations) conditions. Membrane depolarization increases the frequency of fusion events and causes a parallel raise of the net fluorescence signal recorded in whole cell. Single-vesicle analysis reveals modifications of fusion-event behavior (increased peak height and width). These data suggest that potassium depolarization not only induces a massive neurotransmitter release but also modifies the mechanism of vesicle fusion and recycling.
With the appropriate fluorescent probe, this technique can be employed in different cellular systems to dissect the mechanisms of constitutive and stimulated secretion.

This paper provides a method for investigating neurotransmitter vesicle dynamics in neuroblastoma cells, using a synaptobrevin2-pHluorin construct and Total Internal Reflection Fluorescence Microscopy. The strategy developed for image processing and data analysis is also reported.

Synaptic vesicles release neurotransmitters at chemical synapses through a dynamic cycle of fusion and retrieval. Monitoring synaptic activity in real ...

Measuring Synaptic Vesicle Endocytosis in Cultured Hippocampal Neurons

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.

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 ...

Temporal Quantification of MAPK Induced Expression in Single Yeast Cells

The quantification of gene expression at the single cell level uncovers novel regulatory mechanisms obscured in measurements performed at the population level. Two methods based on microscopy and flow cytometry are presented to demonstrate how such data can be acquired. The expression of a fluorescent reporter induced upon activation of the high osmolarity glycerol MAPK pathway in yeast is used as an example. The specific advantages of each method are highlighted. Flow cytometry measures a large number of cells (10,000) and provides a direct measure of the dynamics of protein expression independent of the slow maturation kinetics of the fluorescent protein. Imaging of living cells by microscopy is by contrast limited to the measurement of the matured form of the reporter in fewer cells. However, the data sets generated by this technique can be extremely rich thanks to the combinations of multiple reporters and to the spatial and temporal information obtained from individual cells. The combination of these two measurement methods can deliver new insights on the regulation of protein expression by signaling pathways.

Two complementary methods based on flow cytometry and microscopy are presented which enable the quantification, at the single cell level, of the dynamics of gene expression induced by the activation of a MAPK pathway in yeast.

The quantification of gene expression at the  single cell level uncovers novel regulatory mechanisms obscured in measurements  performed at the population ...

Biology

Imaging FITC-dextran as a Reporter for Regulated Exocytosis

Regulated exocytosis is a process by which cargo, which is stored in secretory granules (SGs), is released in response to a secretory trigger. Regulated exocytosis is fundamental for intercellular communication and is a key mechanism for the secretion of neurotransmitters, hormones, inflammatory mediators, and other compounds, by a variety of cells. At least three distinct mechanisms are known for regulated exocytosis: full exocytosis, where a single SG fully fuses with the plasma membrane, kiss-and-run exocytosis, where a single SG transiently fuses with the plasma membrane, and compound exocytosis, where several SGs fuse with each other, prior to or after SG fusion with the plasma membrane. The type of regulated exocytosis undertaken by a cell is often dictated by the type of secretory trigger. However, in many cells, a single secretory trigger can activate multiple modes of regulated exocytosis simultaneously. Despite their abundance and importance across cell types and species, the mechanisms that determine the different modes of secretion are largely unresolved. One of the main challenges in investigating the different modes of regulated exocytosis, is the difficulty in distinguishing between them as well as exploring them separately. Here we describe the use of fluorescein isothiocyanate (FITC)-dextran as an exocytosis reporter, and live cell imaging, to differentiate between the different pathways of regulated exocytosis, focusing on compound exocytosis, based on the robustness and duration of the exocytic events.

Here we detail a method for live cell imaging of regulated exocytosis. This method utilizes FITC-dextran, which accumulates in lysosome-related organelles, as a reporter. This simple method also allows distinguishing between different modes of regulated exocytosis in cells that are difficult to manipulate genetically.

Regulated exocytosis is a process by which cargo, which is stored in secretory granules (SGs), is released in response to a secretory trigger. Regulated ...

Quantifying Spatiotemporal Parameters of Cellular Exocytosis in Micropatterned Cells

Live imaging of the pHluorin tagged Soluble N-ethylmaleimide-sensitive-factor Attachment protein REceptor (v-SNARE) Vesicle-associated membrane protein 7 (VAMP7) by total internal reflection fluorescence microscopy (TIRFM) is a straightforward way to explore secretion from the lysosomal compartment. Taking advantage of cell culture on micropatterned surfaces to normalize cell shape, a variety of statistical tools were employed to perform a spatial analysis of secretory patterns. Using Ripley&#8217;s K function and a statistical test based on the nearest neighbor distance (NND), we confirmed that secretion from lysosomes is not a random process but shows significant clustering. Of note, our analysis revealed that exocytosis events are also clustered in nonadhesion areas, indicating that adhesion molecules are not the only structures that can induce secretory hot spots at the plasma membrane. Still, we found that cell adhesion enhances clustering. In addition to precisely defined adhesive and nonadhesive areas, the circular geometry of these micropatterns allows the use of polar coordinates, simplifying analyses. We used Kernel Density Estimation (KDE) and the cumulative distribution function on polar coordinates of exocytosis events to identify enriched areas of exocytosis. In ring-shaped micropattern cells, clustering occurred at the border between the adhesive and nonadhesive areas. Our analysis illustrates how statistical tools can be employed to investigate spatial distributions of diverse biological processes.

Live imaging of lysosomal exocytosis on micropatterned cells allows a spatial quantification of this process. Morphology normalization using micropatterns is an outstanding tool to uncover general rules about the spatial distribution of cellular processes.

Live imaging of the pHluorin tagged Soluble N-ethylmaleimide-sensitive-factor Attachment protein REceptor (v-SNARE) Vesicle-associated membrane protein 7 ...

Automated Detection and Analysis of Exocytosis

Timelapse TIRF microscopy of pH-sensitive GFP (pHluorin) attached to vesicle SNARE proteins is an effective method to visualize single vesicle exocytic events in cell culture. To perform an unbiased, efficient identification and analysis of such events, a computer-vision based approach was developed and implemented in MATLAB. The analysis pipeline consists of a cell segmentation and exocytic-event identification algorithm. The computer-vision approach includes tools for investigating multiple parameters of single events, including the half-life of fluorescence decay and peak &#916;F/F, as well as whole-cell analysis of the frequency of exocytosis. These and other parameters of fusion are used in a classification approach to distinguish distinct fusion modes. Here a newly built GUI performs the analysis pipeline from start to finish. Further adaptation of Ripley&#39;s K function in R Studio is used to distinguish between clustered, dispersed, or random occurrence of fusion events in both space and time.

We developed automated computer vision software to detect exocytic events marked by pH-sensitive fluorescent probes. Here, we demonstrate the use of a graphical user interface and RStudio to detect fusion events, analyze and display spatiotemporal parameters of fusion, and classify events into distinct fusion modes.

Timelapse TIRF microscopy of pH-sensitive GFP (pHluorin) attached to vesicle SNARE proteins is an effective method to visualize single vesicle exocytic ...

An Introduction to Endocytosis and Exocytosis

Cells can take in substances from the extracellular environment by endocytosis and actively release molecules into it by exocytosis. Such processes involve lipid membrane-bound sacs called vesicles. Knowledge of the molecular architecture and mechanisms of both is key to understanding normal cell physiology, as well as the disease states that arise when they become defective. This video will first briefly review a few pivotal discoveries in the history of endo- and exocytosis research. Next, some key questions will be examined, followed by a discussion of the prominent methods used to investigate these problems, including cell labeling, fusion assays, and fluorescence imaging. Finally, it will explore current research being conducted by scientists in the field today.

Endocytosis and Exocytosis; Clathrin Coated Pits and SNAREs

Cells can take in substances from the extracellular environment by endocytosis and actively release molecules into it by exocytosis. Such processes ...

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Advanced Biology

Cell Biology

An In Vitro Technique to Visualize Exocytosis of Secretory Granules in Mast Cells

Source: Klein, O., et al. <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/57936">Imaging FITC-dextran as a Reporter for Regulated Exocytosis</a> J. Vis. Exp. (2018).
This video demonstrates a technique to visualize exocytosis in mast cells. The cells are incubated with FITC-dextran &#8212; a fluorescent reporter &#8212; which is taken up by cells inside secretory granules (SGs), where the acidic pH quenches its fluorescence. Upon stimulation of granule exocytosis, the medium&#39;s higher pH induces reporter fluorescence inside the fused SGs, which is visualized using a fluorescence microscope.

1. Preparations

	Preparation of RBL (RBL-2H3 mast cell line) culture media
	
		Mix 500 mL of low glucose Dulbecco&#39;s modified Eagle&#39;s medium ...

Monitoring the Effect of Osmotic Stress on Secretory Vesicles and Exocytosis

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