This work was supported by the Canadian Institutes of Health Research, the Natural Sciences and Engineering Research council (NSERC Discovery Grant) and the Savoy Foundation. OC was supported by a Ph.D. fellowship from NSERC.

All experiments were performed in accordance with the animal welfare guidelines of the Animal Protection Committee of Universit&#233; Laval and the Canadian Council on Animal Care.
1. Preliminary Preparation (Optional: Prepare 1 Day in Advance)
<ol>
	<li>Prepare three types of artificial cerebrospinal fluid (ACSF) solution (Normal, Sucrose and Recovery Solutions, 1 L each; see Table 1). Adjust the osmolality of the solutions to 300 &#177; 10 mOsm25 and cool the ACSF-Sucrose down to a near-freezing point (0-4 &#176;C). 
	NOTE: The use of a low-sodium cutting solution (ACSF-Sucrose) helps preserve the viability of neurons in the superficial layers of acute slices26.</li>
	<li>Prepare 0.75 mL of patch-solution containing a red fluorophore (e.g., Alexa-594) and a green synthetic calcium indicator (e.g., Oregon Green BAPTA-1; see Table 1). Include biocytin (see Table 1) in the patch-solution if post hoc morphological identification of recorded cells is required.</li>
	<li>Adjust the osmolality of the solution to 280 &#177; 5 mOsm and pH to 7.35 &#177; 0.5. Keep the solution in the refrigerator or on ice at all times. 
	NOTE: Choice of the calcium indicator should be predicated on its dynamic range and on the nature of the investigated Ca2+ events.</li>
	<li>Using a micropipette puller, prepare patch pipettes from borosilicate glass capillaries (see Table of Materials) with a &#8776; 2 &#181;m tip (pipette resistance of 3-5 M&#937;) and stimulation pipettes from borosilicate theta-glass capillaries (see Table of Materials) with a 2-5 &#181;m tip. 
	NOTE: The puller settings to make pipettes of a given diameter and shape will be determined by the puller filament type and the ramp test results for a given type of glass.</li>
</ol>
2. Hippocampal Slice Preparation
<ol>
	<li>Anesthetize the mouse (P13-20; the strain and sex of the mouse is determined by the experimental question being addressed) with 1 mL of isoflurane placed onto a paper towel within an inhalation narcosis chamber. When the animal is deeply anesthetized, as evidenced by a lack of movement and slow respiration, remove it from the narcosis chamber and decapitate using a guillotine.</li>
	<li>Expose the skull by cutting the skin with a small pair of scissors from the back of the skull to the nose. Use a small pair of mini bone rongeurs to make a hole at the bregma level. Then use the scissors to make a caudal-to-rostral cut along the sagittal suture. With the rongeurs grasp the back of each skull flap and lift upward and outward to remove the skull covering each hemisphere.</li>
	<li>After the brain is fully exposed, undercut the optic nerves with a small spatula. Remove the brain from the skull and put it into a Petri dish containing continuously oxygenated, cold ACSF-Sucrose (see Table 1 for sucrose concentration).
	<ol>
		<li>If tissue from older mice is required, perform an intracardiac perfusion using a syringe (25G) filled with 20 mL of ice-cold ACSF-Sucrose prior to the brain extraction to obtain good quality slices.</li>
	</ol>
	</li>
	<li>Prepare hippocampal slices from the extracted animal brain.
	<ol>
		<li>Let the brain chill for around 2 min. Place a piece of filter paper on an ice-packed Petri dish, transfer the brain onto the filter paper. Dissect the two hemispheres.</li>
		<li>Glue the dissected hemispheres (the orientation is determined by the experimental goal to obtain coronal, transversal, or horizontal slices) onto a vibratome table and immerse it into the vibratome tray filled with ice-cold oxygenated ACSF-Sucrose. Make 300-&#181;m thick slices at a temperature of about 1 &#176;C by using a vibratome cooler or placing the ice around the vibratome tray.</li>
		<li>Using a flat paint brush, accumulate the slices containing the hippocampus (up to 6 slices per hemisphere) in a bath containing oxygenated ACSF-Recovery heated to 37 &#176;C.</li>
		<li>Leave the slices in the ACSF-Recovery bath for at least 45 min.</li>
	</ol>
	</li>
</ol>
3. Whole-cell Patch-clamp Recordings
<ol>
	<li>Set a hippocampal slice in place in a bath positioned under the objective (magnification: 40x, numerical aperture: 0.8) of a laser-scanning two-photon microscope. Continually perfuse the bath with oxygenated ACSF-Normal heated at 30-32 &#176;C at a rate of 2.5-3 mL/min.</li>
	<li>Use infrared differential interference contrast (IR-DIC) or Dodt-SGC microscopy to locate a cell of interest using its size, shape, and position. 
	NOTE: Depending on the targeted neuron population, a transgenic mouse model can be used to easily locate cells of interest. In this case, this step can be substituted with use of a fluorescent light source.</li>
	<li>Fill a stimulation pipette with an ACSF-Normal solution containing the red fluorophore (e.g., Alexa-594).</li>
	<li>Set the stimulation pipette (connected to an electrical stimulation unit) on top of the slice so that the tip is in the same region as the cell of interest.</li>
	<li>After filling the patch pipette with patch solution and attaching it to a head stage, set it over the slice so that its tip is directly above the cell of interest.</li>
	<li>Fit a syringe into a three-way stopcock and connect it to the patch-pipette through the plastic tube. Inject constant positive pressure into the patch pipette (&#8776; 0.1 mL) using the syringe. Keep the stopcock in &#34;close&#34; position.</li>
	<li>Activate the amplifier control software module and switch to voltage-clamp mode by clicking on the &#34;VC&#34; button. Open the electrophysiology data acquisition software (e.g., clampex) for acquisition of electrophysiological signals and click on the &#34;Membrane Test&#34; icon to have it continually send out a square voltage pulse (5 mV, 10 ms), which is necessary to monitor changes in the pipette resistance.</li>
	<li>Lower the patch pipette until it is right on top of the targeted cell. Upon making contact with the cell membrane, remove the pressure by turning the stopcock into the &#34;open&#34; position. 
	NOTE: Contact with the cell membrane is detected when a small increase in the pipette resistance (&#8776; 0.2 M&#937;) is seen and a small indentation on the cell is caused by positive pressure.</li>
	<li>Apply a slight negative pressure to the patch pipette using an empty syringe fitted into the stopcock until the pipette resistance provided by the software reaches 1 G&#937;. In the &#39;Membrane Test&#39; window of the data acquisition software, clamp the cell at -60 mV.</li>
	<li>Continue applying negative pressure until the cell is opened and the whole-cell configuration is achieved. Detection of this cell state is based upon the sudden change in the pipette resistance (from 1 G&#937; to 70-500 M&#937; depending on the interneuron type) and the appearance of large capacitive transients in the &#39;Membrane Test&#39; window.</li>
</ol>
4. Two-photon Ca2+ Imaging
<ol>
	<li>If interested in the excitatory postsynaptic responses, add the GABAA receptor blocker gabazine (10 &#181;M) and the GABAB receptor blocker CGP55845 (2 &#181;M) in the ACSF bath.</li>
	<li>In amplifier control software module, set the patch configuration to current-clamp by clicking on the &#34;CC&#34; button and record the cell&#39;s firing pattern in response to somatic injections of depolarizing current (0.8-1.0 nA, 1 s). Wait for at least 30 min for the cell to be filled with the indicators present in the patch solution. 
	NOTE: The cell&#39;s firing pattern and active properties can be used to identify the cell&#39;s subtype; e.g., fast-spiking cells. It is important for the indicator concentration to stabilize through diffusion before starting to record CaTs (see Table 2 for troubleshooting).</li>
	<li>AP-evoked CaTs
	<ol>
		<li>Using the image acquisition software, start acquiring images. Locate a dendrite of interest using the red fluorescence signal. To ensure a visible response, first, choose a proximal dendrite (&#8804; 50 &#181;m) as the efficiency of AP backpropagation may significantly decline with distance in GABAergic interneurons22.</li>
		<li>Using the &#39;rectangular tool&#39; in the image acquisition software, zoom in on the targeted region and switch to the &#34;xt&#34; (linescan) mode. Position the scan across the dendritic branch of interest. With the laser intensity controllers in the acquisition software, set the two-photon laser at a minimal power level where baseline green fluorescence is just slightly visible, to avoid phototoxicity.</li>
		<li>In the electrophysiology data acquisition software &#39;Protocol&#39; window and image acquisition software, create a recording trial of the desired duration containing a somatic current injection of the desired amplitude.
		<ol>
			<li>Using the image acquisition software, click the &#34;Start record&#34; button and acquire the fluorescence continuously for 1-2 s. Repeat the image acquisition 3-10 times. Wait at least 30 s between single scans to avoid photodamage. If acquiring linescans at multiple points along a dendrite, take them in random order to avoid order effects.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Synaptically-evoked CaTs
	<ol>
		<li>Locate a dendrite of interest using the red fluorescence signal.</li>
		<li>Set the stimulation pipette on the surface of the slice above the dendrite of interest. Slowly lower the stimulation pipette into place, minimizing movement to avoid disturbing the whole-cell configuration. Position the pipette at 10-15 &#181;m from the dendrite.</li>
		<li>To visualize the location of synaptic microdomains in aspiny dendrites, in the image acquisition software switch to the &#39;xt&#39; (linescan) mode and position the line along the dendritic branch of interest.</li>
		<li>In the &#39;Protocol&#39; Window (of electrophysiology data acquisition software) and image acquisition software, create a recording trial that triggers the stimulation unit after the trial start.</li>
		<li>Using the acquisition software, click the &#34;Start record&#34; button to scan along the dendrite continuously for 1-2 s. Repeat acquisition 3-5 times, waiting 30 s between scans to prevent photodamage. 
		NOTE: The length of scan can be adjusted depending on the evoked event&#39;s kinetics, but should be minimized to prevent photodamage (see Table 2 for troubleshooting).</li>
		<li>Repeat step 4.5.5 in different conditions (e.g., different intensity/length of stimulation, introduction of a pharmacological blocker, etc.) depending on the specific question being addressed.</li>
		<li>Stop the acquisition when the cell shows signs of deteriorating health: depolarization below -45 mV, increase in the baseline Ca2+ level, morphological deterioration of dendrites (e.g., blebbing, fragmentation; see Table 2 for troubleshooting).</li>
		<li>To obtain preliminary information on the cell&#39;s morphology and keep a record of the location of the stimulation pipette, acquire a Z-stack of the cell in the red channel. Using the acquisition software in &#39;xyz&#39; mode, set the upper and lower stack limits to image the entire cell with all processes included. Set the &#39;step size&#39; at 1 &#181;m and initiate the stack acquisition using the &#34;Start record&#34; button.</li>
		<li>When the Z-stack acquisition is complete, use the &#34;Maximum projection&#34; option in the software to superimpose all focal plans of the stack and verify the quality of acquisition. Then, slowly retract the patch pipette out of the slice.</li>
		<li>To fix the slice for post hoc morphological identification, quickly remove the slice from the bath using a flat paint brush, and place it between two filter papers, in an ACSF-filled Petri dish. Replace the ACSF with a 4% paraformaldehyde (PFA) solution and leave the dish in a 4 &#176;C room or refrigerator overnight.</li>
	</ol>
	</li>
</ol>
5. Immunohistochemistry for Post Hoc Morphological Identification of Recorded Cells
NOTE: After 1 night of fixation in PFA, the slice can be stored in phosphate buffer (PB) with sodium azide (0.5%) for up to 1 month.
<ol>
	<li>Put the slice in Tris-buffered saline solution (TBS) with Triton X-100 (0.3%) and perform 4 washes (5-10 min each).</li>
	<li>Put the slice in TBS-Triton 0.3% with 10% normal goat serum (NGS) for 1 h.</li>
	<li>Put the slice in TBS-Triton 0.3% with 1% NGS and a Streptavidin-conjugated fluorophore (e.g., Alexa Fluor 546-conjugated Streptavidin, 1:200) for overnight incubation.</li>
	<li>Wash 4 times (5-10 min) in TBS.</li>
	<li>Mount slices on microscope slides and image using a confocal microscope. To have a complete cell reconstruction, acquire a Z-stack (step size: 1 &#181;m) using a 20x objective. For imaging an Alexa-546-conjugated label, use a 543 nm laser and a 515-560 nm detection filter set.</li>
</ol>
6. Analysis of CaTs
<ol>
	<li>Extract the fluorescence values from the regions of interest (ROIs) in the linescan images from the red and green channels and average the values of the multiple repeats for each condition to reduce noise. 
	NOTE: When linescan acquisition is performed along the dendrite, it is possible to extract data from multiple ROIs, which may correspond to dendritic microdomains (2-5 &#181;m), and thus allowing the study of the Ca2+ signal compartmentalization.</li>
	<li>For each ROI, express the changes in Ca2+ amplitude as: 
	<img alt="Equation" src="/files/ftp_upload/56776/56776eq1.jpg" /> 
	NOTE: Here G is the fluorescence value from the green channel; G0 is the baseline fluorescence value from the green channel during the pre-stimulation period; R is the fluorescence value from the red channel18. As two-photon excitation is highly localized and does not generate a significant background, subtraction of background fluorescence is not required.</li>
</ol>

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The authors have no competing financial interests or other conflicts of interest.

The method shown here demonstrates how the combination of two-photon Ca2+ imaging and patch-clamp electrophysiology can be used for studying dendritic Ca2+ signaling in neuronal dendrites in acute brain slices. This method allows for monitoring of both the local Ca2+ elevations evoked by electrical stimulation or backpropagating AP in dendritic segments, and the cell&#39;s somatic response. This makes it an excellent tool to study how various parts of the dendritic tree integrate inputs a...

The contribution of a neuron to network activity is largely determined by the dynamic nature of the synaptic inputs it receives. Traditionally, the predominant method of characterizing synaptic activity in neurons relied on somatic whole-cell patch-clamp recordings of postsynaptic currents evoked by electrical stimulation of axons of passage. However, only activity of the proximally located synapses is truthfully reported in this case1. In addition, to assess the synapse-specific mechanisms, recordings from pairs of neurons and from dendrites at a specific location have been used to target the synapses of interest and the mechanisms of dendritic integration, respectively. A major breakthrough in the field of synaptic physiology was achieved through a marriage of optical and electrophysiological techniques. Two-photon excitation laser scanning microscopy (2PLSM) in combination with Ca2+ imaging and optogenetic tools can reveal tremendous details of the dynamic organization of synaptic activity at specific neuronal connections in brain slices in vitro and in vivo.
Several key advantages made 2PLSM stand out from the conventional, one-photon excitation microscopy2: (1) due to a nonlinear nature of two-photon excitation, the fluorescence is generated only in the focal volume, and all emitted photons represent useful signals (no need for pinhole); (2) longer wavelengths, used in 2PLSM, penetrate the scattering tissue more efficiently; in addition, scattered photons are too dilute to produce two-photon excitation and background fluorescence; (3) photodamage and phototoxicity are also limited to the focal plane. Therefore, despite the high cost of 2-photon systems in comparison with conventional confocal microscopes, the 2PLSM remains a method of choice for high-resolution investigation of neuronal structure and function in thick living tissue.
The first application of 2PLSM in scattering tissue was to image the structure and function of dendritic spines3. 2PLSM in combination with Ca2+ imaging has revealed that spines function as isolated biochemical compartments. Since in many neuronal types there is a one-to-one correspondence between spines and individual synapses4, two-photon Ca2+ imaging soon became a useful tool reporting the activity of individual synapses in intact tissue5,6,7,8. Furthermore, 2PLSM-based Ca2+ imaging was successfully used to monitor the activity of single calcium channels and the nonlinear interactions between the intrinsic and synaptic conductances, as well as to assess the state- and activity-dependent regulation of Ca2+ signaling in neuronal dendrites5,6,7,8,9,10,11.
Calcium is a ubiquitous intracellular second messenger, and its subcellular spatiotemporal organization determines the direction of physiological reactions, from changes in synaptic strength to the regulation of ion channels, dendrite and spine growth, as well as cell death and survival. Dendritic Ca2+ elevations occur via activation of multiple pathways. Action potentials (APs), backpropagating to the dendrites, open voltage-gated calcium channels12 and produce relatively global Ca2+ transients (CaTs) in dendrites and spines13. Synaptic transmission is associated with activation of postsynaptic Ca2+-permeable receptors (NMDA, Ca2+-permeable AMPA and kainate), triggering synaptic CaTs6,14,15. Finally, supralinear Ca2+ events can be generated in dendrites under certain conditions11,12,13,16.
Two-photon Ca2+ imaging in combination with patch-clamp electrophysiological recordings employs synthetic Ca2+-sensitive fluorescent indicators, which are typically delivered through the patch electrode during whole-cell recordings. A standard method for quantification of Ca2+ dynamics is based on the dual indicator method17,18. It uses two fluorophores with well separated emission spectra (e.g., a combination of a red Ca2+-insensitive dye with green Ca2+ indicators, such as Oregon Green BAPTA-1 or Fluo-4) and has several advantages when compared to the single indicator method. First, a Ca2+-insensitive dye is used to locate small structures of interest (dendritic branches and spines) where Ca2+ imaging will be performed. Second, the ratio between the change in green and red fluorescence (&#916;G/R) is calculated as a measure of [Ca2+], which is largely insensitive to changes in baseline fluorescence due to fluctuations in [Ca2+]017,18. Furthermore, fluorescence changes can be calibrated in terms of absolute Ca2+ concentrations19.
A general concern when running two-photon Ca2+ imaging experiments in acute slices is cell health and stability of the image acquisition due to the high laser power typically used. Additionally, in Ca2+ imaging experiments, there is concern about the perturbation and substantial overestimation of subcellular Ca2+ dynamics due to the fact that Ca2+ indicators act as highly mobile exogenous Ca2+ buffers. Thus, the choice of the Ca2+ indicator and its concentration depends on the neuronal type, the anticipated amplitude of CaTs, and on the experimental question.
We adapted the method of two-photon Ca2+ imaging for investigation of Ca2+ fluctuations in dendrites of GABAergic interneurons9,10,11,20,21,22. While the bulk of early Ca2+ imaging studies were done in principal neurons, inhibitory interneurons showcase a large variety of functional Ca2+ mechanisms that are distinct from those in pyramidal cells20,23,24. These interneuron-specific mechanisms (e.g., Ca2+ permeable AMPA receptors) may play specific roles in regulating cell activity. While dendritic Ca2+ signaling in interneurons is a tempting target for further investigation, two-photon Ca2+ imaging in dendrites of these cells presents additional challenges, from a thinner diameter of dendrites and lack of spines to a particularly high endogenous Ca2+ binding capacity. As our research interests focus on the study of hippocampal interneurons, the following protocol, while applicable to different neuronal populations, was adapted to deal with those challenges.
This protocol was executed with a commercial confocal two-photon microscope, which was equipped with two external, non-descanned detectors (NDDs), electro-optical modulator (EOM), and a Dodt scanning gradient contrast (SGC), and installed on an optical table. The microscope was coupled with a Ti:Sapphire multiphoton laser mode-locked at 800 nm (&#62; 3 W, 140 fs pulses, 80 Hz repetition rate). The imaging system was equipped with a standard electrophysiology rig, including a perfusion chamber with temperature control, a translating platform with two micromanipulators, a computer-controlled microelectrode amplifier, a digitizer, a stimulation unit, and data acquisition software.

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two-photon calcium imaging in neuronal dendrites in brain slices

Calcium (Ca2+) imaging is a powerful tool to investigate the spatiotemporal dynamics of intracellular Ca2+ signals in neuronal dendrites. Ca2+ fluctuations can occur through a variety of membrane and intracellular mechanisms and play a crucial role in the induction of synaptic plasticity and regulation of dendritic excitability. Hence, the ability to record different types of Ca2+ signals in dendritic branches is valuable for groups studying how dendrites integrate information. The advent of two-photon microscopy has made such studies significantly easier by solving the problems inherent to imaging in live tissue, such as light scattering and photodamage. Moreover, through combination of conventional electrophysiological techniques with two-photon Ca2+ imaging, it is possible to investigate local Ca2+ fluctuations in neuronal dendrites in parallel with recordings of synaptic activity in soma. Here, we describe how to use this method to study the dynamics of local Ca2+ transients (CaTs) in dendrites of GABAergic inhibitory interneurons. The method can be also applied to studying dendritic Ca2+ signaling in different neuronal types in acute brain slices.

Using the protocol presented here, we obtained CaTs evoked by somatic current injection and by electrical stimulation in dendrites of oriens/alveus interneurons in the CA1 area of the hippocampus. After patching a neuron, identified based on its shape and position, we acquired linescans across a proximal dendrite at multiple points at given distances from the soma (Figure 1A). We observed a decrease in the amplitude of CaTs induced by backpropagating APs as t...

Watch this Scientific Journal Video about Two-photon Calcium Imaging in Neuronal Dendrites in Brain Slices at JoVE.com

Two-photon Calcium Imaging in Neuronal Dendrites in Brain Slices

We present a method combining whole-cell patch-clamp recordings and two-photon imaging to record Ca2+ transients in neuronal dendrites in acute brain slices.

Calcium (Ca2+) imaging is a powerful tool to investigate the spatiotemporal dynamics of intracellular Ca2+ signals in neuronal dendrites. Ca2+ ...

two-photon-calcium-imaging-in-neuronal-dendrites-in-brain-slices

Universidad de Cartagena UDEC

Research

JoVE Journal

Neuroscience

10.6K Views.  Université Laval. We present a method combining whole-cell patch-clamp recordings and two-photon imaging to record Ca2+ transients in neuronal dendrites in acute brain slices.

Video: Two-photon Calcium Imaging in Neuronal Dendrites in Brain Slices

Imaging Calcium Responses in GFP-tagged Neurons of Hypothalamic Mouse Brain Slices

Despite an enormous increase in our knowledge about the mechanisms underlying the encoding of information in the brain, a central question concerning the precise molecular steps as well as the activity of specific neurons in multi-functional nuclei of brain areas such as the hypothalamus remain. This problem includes identification of the molecular components involved in the regulation of various neurohormone signal transduction cascades. Elevations of intracellular Ca2+ play an important role in regulating the sensitivity of neurons, both at the level of signal transduction and at synaptic sites.
New tools have emerged to help identify neurons in the myriad of brain neurons by expressing green fluorescent protein (GFP) under the control of a particular promoter. To monitor both spatially and temporally stimulus-induced Ca2+ responses in GFP-tagged neurons, a non-green fluorescent Ca2+ indicator dye needs to be used. In addition, confocal microscopy is a favorite method of imaging individual neurons in tissue slices due to its ability to visualize neurons in distinct planes of depth within the tissue and to limit out-of-focus fluorescence. The ratiometric Ca2+ indicator fura-2 has been used in combination with GFP-tagged neurons1. However, the dye is excited by ultraviolet (UV) light. The cost of the laser and the limited optical penetration depth of UV light hindered its use in many laboratories. Moreover, GFP fluorescence may interfere with the fura-2 signals2. Therefore, we decided to use a red fluorescent Ca2+ indicator dye. The huge Stokes shift of fura-red permits multicolor analysis of the red fluorescence in combination with GFP using a single excitation wavelength. We had previously good results using fura-red in combination with GFP-tagged olfactory neurons3. The protocols for olfactory tissue slices seemed to work equally well in hypothalamic neurons4. Fura-red based Ca2+ imaging was also successfully combined with GFP-tagged pancreatic &beta;-cells and GFP-tagged receptors expressed in HEK cells5,6. A little quirk of fura-red is that its fluorescence intensity at 650 nm decreases once the indicator binds calcium7. Therefore, the fluorescence of resting neurons with low Ca2+ concentration has relatively high intensity. It should be noted, that other red Ca2+-indicator dyes exist or are currently being developed, that might give better or improved results in different neurons and brain areas.

In this protocol, we update recent progress in imaging Ca2+ signals of GFP-tagged neurons in brain tissue slices using a red fluorescent Ca2+ indicator dye.

Despite an enormous increase in our knowledge about the mechanisms underlying the encoding of information in the brain, a central question concerning the ...

Dual Electrophysiological Recordings of Synaptically-evoked Astroglial and Neuronal Responses in Acute Hippocampal Slices

Astrocytes form together with neurons tripartite synapses, where they integrate and modulate neuronal activity. Indeed, astrocytes sense neuronal inputs through activation of their ion channels and neurotransmitter receptors, and process information in part through activity-dependent release of gliotransmitters. Furthermore, astrocytes constitute the main uptake system for glutamate, contribute to potassium spatial buffering, as well as to GABA clearance. These cells therefore constantly monitor synaptic activity, and are thereby sensitive indicators for alterations in synaptically-released glutamate, GABA and extracellular potassium levels. Additionally, alterations in astroglial uptake activity or buffering capacity can have severe effects on neuronal functions, and might be overlooked when characterizing physiopathological situations or knockout mice. Dual recording of neuronal and astroglial activities is therefore an important method to study alterations in synaptic strength associated to concomitant changes in astroglial uptake and buffering capacities. Here we describe how to prepare hippocampal slices, how to identify stratum radiatum astrocytes, and how to record simultaneously neuronal and astroglial electrophysiological responses. Furthermore, we describe how to isolate pharmacologically the synaptically-evoked astroglial currents.

The preparation of acute brain slices from isolated hippocampi, as well as the simultaneous electrophysiological recordings of astrocytes and neurons in stratum radiatum during stimulation of schaffer collaterals is described. The pharmacological isolation of astroglial potassium and glutamate transporter currents is demonstrated.

Astrocytes form together with neurons tripartite synapses, where they integrate and modulate neuronal activity. Indeed, astrocytes sense neuronal inputs ...

In Vivo Two-photon Imaging Of Experience-dependent Molecular Changes In Cortical Neurons

The brain's ability to change in response to experience is essential for healthy brain function, and abnormalities in this process contribute to a variety of brain disorders1,2. To better understand the mechanisms by which brain circuits react to an animal's experience requires the ability to monitor the experience-dependent molecular changes in a given set of neurons, over a prolonged period of time, in the live animal. While experience and associated neural activity is known to trigger gene expression changes in neurons1,2, most of the methods to detect such changes do not allow repeated observation of the same neurons over multiple days or do not have sufficient resolution to observe individual neurons3,4. Here, we describe a method that combines in vivo two-photon microscopy with a genetically encoded fluorescent reporter to track experience-dependent gene expression changes in individual cortical neurons over the course of day-to-day experience. 
One of the well-established experience-dependent genes is Activity-regulated cytoskeletal associated protein (Arc)5,6. The transcription of Arc is rapidly and highly induced by intensified neuronal activity3, and its protein product regulates the endocytosis of glutamate receptors and long-term synaptic plasticity7. The expression of Arc has been widely used as a molecular marker to map neuronal circuits involved in specific behaviors3. In most of those studies, Arc expression was detected by in situ hybridization or immunohistochemistry in fixed brain sections. Although those methods revealed that the expression of Arc was localized to a subset of excitatory neurons after behavioral experience, how the cellular patterns of Arc expression might change with multiple episodes of repeated or distinctive experiences over days was not investigated. 
In vivo two-photon microscopy offers a powerful way to examine experience-dependent cellular changes in the living brain8,9. To enable the examination of Arc expression in live neurons by two-photon microscopy, we previously generated a knock-in mouse line in which a GFP reporter is placed under the control of the endogenous Arc promoter10. This protocol describes the surgical preparations and imaging procedures for tracking experience-dependent Arc-GFP expression patterns in neuronal ensembles in the live animal. In this method, chronic cranial windows were first implanted in Arc-GFP mice over the cortical regions of interest. Those animals were then repeatedly imaged by two-photon microscopy after desired behavioral paradigms over the course of several days. This method may be generally applicable to animals carrying other fluorescent reporters of experience-dependent molecular changes4.

In Vivo Two-photon Imaging Of Experience-dependent Molecular Changes In Cortical Neurons

Experience-dependent molecular changes in neurons are essential for the brain's ability to adapt in response to behavioral challenges. An in vivo two-photon imaging method is described here that allows the tracking of such molecular changes in individual cortical neurons through genetically encoded reporters.

The brain's ability to change in response to experience is essential for healthy brain function, and abnormalities in this process contribute to a variety ...

In vivo Neuronal Calcium Imaging in C. elegans

The nematode worm C. elegans is an ideal model organism for relatively simple, low cost neuronal imaging in vivo. Its small transparent body and simple, well-characterized nervous system allows identification and fluorescence imaging of any neuron within the intact animal. Simple immobilization techniques with minimal impact on the animal's physiology allow extended time-lapse imaging. The development of genetically-encoded calcium sensitive fluorophores such as cameleon 1 and GCaMP 2 allow in vivo imaging of neuronal calcium relating both cell physiology and neuronal activity. Numerous transgenic strains expressing these fluorophores in specific neurons are readily available or can be constructed using well-established techniques. Here, we describe detailed procedures for measuring calcium dynamics within a single neuron in vivo using both GCaMP and cameleon. We discuss advantages and disadvantages of both as well as various methods of sample preparation (animal immobilization) and image analysis. Finally, we present results from two experiments: 1) Using GCaMP to measure the sensory response of a specific neuron to an external electrical field and 2) Using cameleon to measure the physiological calcium response of a neuron to traumatic laser damage. Calcium imaging techniques such as these are used extensively in C. elegans and have been extended to measurements in freely moving animals, multiple neurons simultaneously and comparison across genetic backgrounds. C. elegans presents a robust and flexible system for in vivo neuronal imaging with advantages over other model systems in technical simplicity and cost.

In vivo Neuronal Calcium Imaging in C. elegans

With its small transparent body, well-documented neuroanatomy and a host of amenable genetic techniques and reagents, C. elegans makes an ideal model organism for in vivo neuronal imaging using relatively simple, low-cost techniques. Here we describe single neuron imaging within intact adult animals using genetically encoded fluorescent calcium indicators.

The nematode worm C. elegans is an ideal model organism  for relatively simple, low cost neuronal imaging in vivo. Its small transparent body and simple, ...

Two-photon Imaging of Cellular Dynamics in the Mouse Spinal Cord

Two-photon (2P) microscopy is utilized to reveal cellular dynamics and interactions deep within living, intact tissues. Here, we present a method for live-cell imaging in the murine spinal cord. This technique is uniquely suited to analyze neural precursor cell (NPC) dynamics following transplantation into spinal cords undergoing neuroinflammatory demyelinating disorders. NPCs migrate to sites of axonal damage, proliferate, differentiate into oligodendrocytes, and participate in direct remyelination. NPCs are thereby a promising therapeutic treatment to ameliorate chronic demyelinating diseases. Because transplanted NPCs migrate to the damaged areas on the ventral side of the spinal cord, traditional intravital 2P imaging is impossible, and only information on static interactions was previously available using histochemical staining approaches. Although this method was generated to image transplanted NPCs in the ventral spinal cord, it can be applied to numerous studies of transplanted and endogenous cells throughout the entire spinal cord. In this article, we demonstrate the preparation and imaging of a spinal cord with enhanced yellow fluorescent protein-expressing axons and enhanced green fluorescent protein-expressing transplanted NPCs.

A new ex vivo preparation for imaging the mouse spinal cord. This protocol allows for two-photon imaging of live cellular interactions throughout the spinal cord.

Two-photon (2P) microscopy is utilized to reveal cellular dynamics and interactions deep within living, intact tissues. Here, we present a method for ...

In Vivo Functional Brain Imaging Approach Based on Bioluminescent Calcium Indicator GFP-aequorin

Functional in vivo imaging has become a powerful approach to study the function and physiology of brain cells and structures of interest. Recently a new method of Ca2+-imaging using the bioluminescent reporter GFP-aequorin (GA) has been developed. This new technique relies on the fusion of the GFP and aequorin genes, producing a molecule capable of binding calcium and&#160;&#8212; with the addition of its cofactor coelenterazine &#8212; emitting bright light that can be monitored through a photon collector. Transgenic lines carrying the GFP-aequorin gene have been generated for both mice and Drosophila. In Drosophila, the GFP-aequorin gene has been placed under the control of the GAL4/UAS binary expression system allowing for targeted expression and imaging within the brain. This method has subsequently been shown to be capable of detecting both inward Ca2+-transients and Ca2+-released from inner stores. Most importantly it allows for a greater duration in continuous recording, imaging at greater depths within the brain, and recording at high temporal resolutions (up to 8.3 msec). Here we present the basic method for using bioluminescent imaging to record and analyze Ca2+-activity within the mushroom bodies, a structure central to learning and memory in the fly brain.

In Vivo Functional Brain Imaging Approach Based on Bioluminescent Calcium Indicator GFP-aequorin

Here we present a novel Ca2+-imaging approach using a bioluminescent reporter. This approach uses a fused construct GFP-aequorin which binds to Ca2+ and emits light, eliminating the need for light excitation. Significantly this method permits long continuous imaging, access to deep brain structures and high temporal resolution.

Functional in vivo imaging has become a powerful approach to study the function and physiology of brain cells and structures of interest. Recently a new ...

Ablation of a Neuronal Population Using a Two-photon Laser and Its Assessment Using Calcium Imaging and Behavioral Recording in Zebrafish Larvae

To identify the role of a subpopulation of neurons in behavior, it is essential to test the consequences of blocking its activity in living animals. Laser ablation of neurons is an effective method for this purpose when neurons are selectively labeled with fluorescent probes. In the present study, protocols for laser ablating a subpopulation of neurons using a two-photon microscope and testing of its functional and behavioral consequences are described. In this study, prey capture behavior in zebrafish larvae is used as a study model. The pretecto-hypothalamic circuit is known to underlie this visually-driven prey catching behavior. Zebrafish pretectum were laser-ablated, and neuronal activity in the inferior lobe of the hypothalamus (ILH; the target of the pretectal projection) was examined. Prey capture behavior after pretectal ablation was also tested.

Here, we present a protocol to ablate a genetically labeled subpopulation of neurons by a two-photon laser from Zebrafish larvae.

To identify the role of a subpopulation of neurons in behavior, it is essential to test the consequences of blocking its activity in living animals. Laser ...

In Vivo Two-photon Imaging of Cortical Neurons in Neonatal Mice

Two-photon imaging is a powerful tool for the in vivo analysis of neuronal circuits in the mammalian brain. However, a limited number of in vivo imaging methods exist for examining the brain tissue of live newborn mammals. Herein we summarize a protocol for imaging individual cortical neurons in living neonatal mice. This protocol includes the following two methodologies: (1) the Supernova system for sparse and bright labeling of cortical neurons in the developing brain, and (2) a surgical procedure for the fragile neonatal skull. This protocol allows the observation of temporal changes of individual cortical neurites during neonatal stages with a high signal-to-noise ratio. Labeled cell-specific gene silencing and knockout can also be achieved by combining the Supernova with RNA interference and CRISPR/Cas9 gene editing systems. This protocol can, thus, be used for analyzing the developmental dynamics of cortical neurons, molecular mechanisms that control the neuronal dynamics, and changes in neuronal dynamics in disease models.

In Vivo Two-photon Imaging of Cortical Neurons in Neonatal Mice

We present an in vivo two-photon imaging protocol for imaging the cerebral cortex of neonatal mice. This method is suitable for analyzing the developmental dynamics of cortical neurons, the molecular mechanisms that control the neuronal dynamics, and the changes in neuronal dynamics in disease models.

Two-photon imaging is a powerful tool for the in vivo analysis of neuronal circuits in the mammalian brain. However, a limited number of in vivo imaging ...

Two-photon Imaging of Microglial Processes' Attraction Toward ATP or Serotonin in Acute Brain Slices

Microglial cells are resident innate immune cells of the brain that constantly scan their environment with their long processes and, upon disruption of homeostasis, undergo rapid morphological changes. For example, a laser lesion induces in a few minutes an oriented growth of microglial processes, also called &#34;directional motility&#34;, toward the site of injury. A similar effect can be obtained by delivering locally ATP or serotonin (5-hydroxytryptamine [5-HT]). In this article, we describe a protocol to induce a directional growth of microglial processes toward a local application of ATP or 5-HT in acute brain slices of young and adult mice and to image this attraction over time by multiphoton microscopy. A simple method of quantification with free and open-source image analysis software is proposed. A challenge that still characterizes acute brain slices is the limited time, decreasing with age, during which the cells remain in a physiological state. This protocol, thus, highlights some technical improvements (medium, air-liquid interface chamber, imaging chamber with a double perfusion) aimed at optimizing the viability of microglial cells over several hours, especially in slices from adult mice.

Microglia, the resident immune cells of the brain, respond quickly with morphological changes to modifications of their environment. This protocol describes how to use two-photon microscopy to study the attraction of microglial processes toward serotonin or ATP in acute brain slices of mice.

Microglial cells are resident innate immune cells of the brain that constantly scan their environment with their long processes and, upon disruption of ...

Transpupillary Two-Photon In Vivo Imaging of the Mouse Retina

The retina transforms light signals from the environment into electrical signals that are propagated to the brain. Diseases of the retina are prevalent and cause visual impairment and blindness. Understanding how such diseases progress is critical to formulating new treatments. In vivo&#160;microscopy in animal models of disease is a powerful tool for understanding neurodegeneration and has led to important progress towards treatments of conditions ranging from Alzheimer&#39;s disease to stroke. Given that the retina is the only central nervous system structure inherently accessible by optical approaches, it naturally lends itself towards in vivo imaging. However, the native optics of the lens and cornea present some challenges for effective imaging access.
This protocol outlines methods for in vivo two-photon imaging of cellular cohorts and structures in the mouse retina at cellular resolution, applicable for both acute- and chronic-duration imaging experiments. It presents examples of retinal ganglion cell (RGC), amacrine cell, microglial, and vascular imaging using a suite of labeling techniques including adeno-associated virus (AAV) vectors, transgenic mice, and inorganic dyes. Importantly, these techniques extend to all cell types of the retina, and suggested methods for accessing other cellular populations of interest are described. Also detailed are example strategies for manual image postprocessing for display and quantification. These techniques are directly applicable to studies of retinal function in health and disease.

In vivo imaging is a powerful tool for the study of biology in health and disease. This protocol describes transpupillary imaging of the mouse retina with a standard two-photon microscope. It also demonstrates different in vivoimaging methods to fluorescently label multiple cellular cohorts of the retina.

The retina transforms light signals from the environment into electrical signals that are propagated to the brain. Diseases of the retina are prevalent ...

Two-photon Calcium Imaging in Neuronal Dendrites in Brain Slices

Summary

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Chapters in this video

Imaging Calcium Responses in GFP-tagged Neurons of Hypothalamic Mouse Brain Slices

Dual Electrophysiological Recordings of Synaptically-evoked Astroglial and Neuronal Responses in Acute Hippocampal Slices

In Vivo Two-photon Imaging Of Experience-dependent Molecular Changes In Cortical Neurons

In vivo Neuronal Calcium Imaging in C. elegans

Two-photon Imaging of Cellular Dynamics in the Mouse Spinal Cord

In Vivo Functional Brain Imaging Approach Based on Bioluminescent Calcium Indicator GFP-aequorin

Ablation of a Neuronal Population Using a Two-photon Laser and Its Assessment Using Calcium Imaging and Behavioral Recording in Zebrafish Larvae

In Vivo Two-photon Imaging of Cortical Neurons in Neonatal Mice

Two-photon Imaging of Microglial Processes' Attraction Toward ATP or Serotonin in Acute Brain Slices

Transpupillary Two-Photon In Vivo Imaging of the Mouse Retina