Name: biocytin recovery and 3d reconstructions of filled hippocampal ca2 interneurons
Uploaded: 2018-11-20T14:45:00.000+00:00
Duration: 11 min 21 s
Description: Watch this Scientific Journal Video about Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons at JoVE.com

This research has received funding from Novartis Pharma (Basel) and the Medical Research Council awarded to Prof Alex Thomson, the Biotechnology and Biological Sciences Research Council (BBSRC- BB/G008639/1), the Physiological Society, the European Union&#39;s Horizon 2020 Framework Programme for Research and Innovation under the Specific Grant Agreement No. 720270 (Human Brain Project SGA1) and under the Specific Grant Agreement No. 785907 (Human Brain Project SGA2). We are extremely grateful to Prof Alex Thomson for setting up the protocol in other cortical regions, securing funding and for her continuous support for this project. Contributions made by lab-members who helped optimising the recovery protocol and reconstructed CA2 neurones are gratefully acknowledged: J. Deuchars, H. Pawelzik, D. I. Hughes, A. P. Bannister, K. Eastlake, H. Trigg, N. A. Botcher.

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The authors have nothing to disclose.

Electrophysiological recordings in vitro (Figure 1 Ac,d and Bc,d) combined with histochemical and immunohistochemical procedures enable the detailed morphology, calcium binding protein content and identity of adult cortical interneurons recorded to be revealed. In the CA2 region, this technique allowed the study of the local circuitry for the first time and revealed subclasses of interneurons that had not been previously described in CA1 or CA3: wide dendritic and axonal arbor basket cells (Figure 1B), bistratified cells and SP-SR interneurons.
The protocol described here has been optimized to preserve the ultrastructure of the neurons and obtain excellent recovery of both dendritic (including spines) and axonal arbors. Critical steps includes the use of the double fixation technique to enhance contrast for light microscopy26 and the addition of glutaraldehyde and picric acid solution to the fixative solution to enhance antibody penetration and preserve the neuronal ultrastructure27. Gentle freeze-thaw permeabilization gives better preservation of fine structure, while osmication and resin embedding reduce z-plane shrinkage28. In addition, the visualization of very fine structures (fine axons with small boutons for example) is improved by incubating the sections with H2O2 and NaBH4 to reduce background staining. Contrast can also be increased with the addition of NiCl2 to the HRP reaction.
The histological procedure detailed here offers excellent results in terms of reproducibility and reliability. However, the duration of the electrophysiological recordings will determine the quality of the biocytin/fluorescence staining, with shorter recordings usually associated with poor axonal staining. The choice of recording protocols (intracellular recordings using sharp electrodes vs. whole-cell patch clamping) may also influence biocytin retention and preservation of fine anatomy.
While the difficulties encountered in preserving fine structure during histological processing described here and the time taken to reconstruct at 100X magnification (1-4weeks depending on the complexity of the axon) are appreciated, this method gives an accurate representation of dendritic and axonal diameters. The use of less demanding protocols to reveal biocytin-labelling is understandable, however, these often preclude clear visualization of fine axonal branches. Detergents, to promote entry of Avidin-HRP to reveal the biocytin and antibodies, are often necessary in thick sections, but can disrupt fine structure. Neuroscientists search constantly for semiautomatic methods of reconstruction, but, for now and for axons especially, biocytin-HRP with manual reconstruction remains the gold standard31.
Highly detailed neuronal reconstructions, especially accurate drawings of axonal boutons and nodes, the presence or absence of myelin and more generally the drawing of complete axonal arbor, with the representation of accurate axon-diameter changes along its length, provide further information for accurate identification of a distinct type of interneurone. Although many interneurons may not fit exactly into a specific class, the technique described above provides correlated data on neuronal electrophysiological properties, the short-term plasticity associated with a specific type of connection and detailed neuronal reconstructions, allowing the wiring diagram, in the CA2 region, for example, to be studied in detail.
Fine, detailed structure is often simplified in computational models. While understandable, this results in the loss of the information that could prove critical in the future. Analysis of detailed 3D reconstructions with parallel synaptic data will allow the addition of further criteria for interneuronal classification. Data can be deposited in public repositories and used by modellers to explore the outcome of sporadic changes in axon diameter and myelination on action potential propagation computationally.

The cortex and hippocampus are structures of such complexity that the classification of neuronal subtypes1,2,3,4, maps of the connections between them5,6,7,8,9,10,11 and how this circuitry supports cognitive functions12,13,14,15 are still under intense study and the subject of continuing debate. For example, to understand the details and complexities of the circuitry and to coordinate data obtained from many different studies, it is extremely helpful to be able to define and describe the components, but it remains a matter for debate how many different classes of neurons exist, or even whether it is possible to define all neurons as belonging to a specific class. Computational tools that can build and test circuits with varying degrees of complexity are being developed16,17,18, but central to these endeavors is the need for detailed studies of the cell types and of the properties of the connections between them. A large amount of information about the local circuitry of the neocortex of adult rats has already been collected using the protocol described here10,19,20,21,22. Although the &#34;wiring diagram&#34; is far from complete, some clear patterns or rules have emerged. Moreover, although some details vary, these rules are common to two mammalian species (rat and cat) and across several neocortical regions, allowing the development of basic building blocks that are likely to be equally applicable to human neocortex. The technique described here is used to extend our understanding of the functional map of cortical circuitry by identifying the presynaptic and postsynaptic neurons involved in connections in the regions that have not been studied in detail before, using a protocol that allows excellent tissue preservation and remarkable staining recovery in adult brain tissue. Data on the local circuitry in CA2 and neuronal properties in this subfield have been collected with this method by combining intracellular electrophysiological recordings (paired recordings with sharp microelectrodes) with biocytin filling, immunofluorescence, histological procedures and highly-detailed neuronal reconstructions, allowing direct comparison with the neighboring CA regions23,24,25.
The technique described in this article has been developed over the years to obtain detailed neuronal anatomy allowing the correct classification of the cells and high quality and accurate reconstructions of both their dendritic and axonal arbors, data that can be correlated with electrophysiological data collected from paired recordings using sharp electrodes. The histological protocol has been optimized to preserve the ultrastructure of the neurons and obtain excellent recovery of both dendritic (including spines) and axonal arbors. For example, the principle of the double fixation technique by firstly immersing in a fixative solution and secondly post-fixing in osmium tetroxide gives a good contrast for light microscopy26. A small amount of glutaraldehyde and picric acid solution are added to the fixative solution to enhance antibody penetration and to preserve the cells&#39; ultrastructure as suggested in a previous study27. The permeabilization of the brain slices using the freeze-thaw method combined with cryo-protection with sucrose, rather than a traditional detergent, also provides optimal preservation of the tissues for detailed morphological analysis of the recorded cells. In addition, the visualization particularly of very fine structures is improved by reducing background staining, with the incubations with hydrogen peroxide (H2O2) and sodium borohydride (NaBH4). Adding nickel chloride (NiCl2) to the horseradish peroxidase (HRP) reaction to obtain a black pigment reaction product also increases the contrast.
The following protocol describes the procedures used to ascertain excellent tissue preservation and highly detailed neuronal&#160;3D reconstructions following intracellular recordings in vitro. The description of the slice preparation, intracellular paired recordings using sharp electrodes and subsequent histological procedures used in our laboratory have been previously reported28. Although the protocol applies to the cells filled intracellularly with biocytin in 450&#8211;500 &#956;m thick slices, the same protocol may be used following whole-cell recordings. However, the use of thinner slices will result in less complete reconstructions of the cells.

<table><tbody><tr><td>Avidin-7-amino-4-methylcoumarin-3-acetic acid (Avidin-AMCA) antibody- 20.8 mg/mL&amp;nbsp;</td><td>Vector laboratories</td><td>A2008</td><td></td></tr><tr><td>Biocytin&amp;nbsp; &amp;ge;98% (TLC)</td><td>Sigma</td><td>B4261</td><td></td></tr><tr><td>3,5 diaminobenzidine (DAB) tablet, To prepare 5 mL</td><td>Sigma</td><td>D4293</td><td></td></tr><tr><td>Durcupan epoxy resin A</td><td>Sigma</td><td>44611</td><td></td></tr><tr><td>Durcupan epoxy resin B</td><td>Sigma</td><td>44612</td><td></td></tr><tr><td>Durcupan epoxy resin C</td><td>Sigma</td><td>44613</td><td></td></tr><tr><td>Durcupan epoxy resin D</td><td>Sigma</td><td>44614</td><td></td></tr><tr><td>Ethanol, puriss. p.a., absolute, &amp;ge;99.8%</td><td>Sigma</td><td>32221</td><td></td></tr><tr><td>Gelatin</td><td>Sigma</td><td>48723</td><td></td></tr><tr><td>Glutaraldehyde solution, grade I, 25 % in H&lt;sub&gt;2&lt;/sub&gt;O</td><td>Sigma</td><td>G5882</td><td></td></tr><tr><td>Glycerol, &amp;ge;99%&amp;nbsp;</td><td>Sigma</td><td>G5516</td><td></td></tr><tr><td>Goat serum</td><td>Sigma</td><td>G9023</td><td></td></tr><tr><td>Goat anti-mouse fluorescein isothiocyanate (FITC)- 14.3 mg/mL</td><td>Sigma</td><td>F2653</td><td></td></tr><tr><td>Goat anti-rabbit Texas Red (TR)- 3.3 mg/mL</td><td>Invitrogen</td><td>T2767</td><td></td></tr><tr><td>Hydrogen peroxide, 30% solution</td><td>Sigma</td><td>H-1009</td><td></td></tr><tr><td>Immersion oil, viscosity 1.250 cSt (lit.)</td><td>Sigma</td><td>I0890</td><td></td></tr><tr><td>Nickel chloride (NiCl&lt;sub&gt;2&lt;/sub&gt; . 6H&lt;sub&gt;2&lt;/sub&gt;O)</td><td>Sigma&amp;nbsp;</td><td>N5756</td><td></td></tr><tr><td>Osmium tetroxide, for electron microscopy, 4% in H&lt;sub&gt;2&lt;/sub&gt;O&amp;nbsp;</td><td>Sigma</td><td>75632</td><td></td></tr><tr><td>Paraformaldehyde, reagent grade, crystalline&amp;nbsp;</td><td>Sigma</td><td>P6148</td><td></td></tr><tr><td>Picric acid, moistened with water, &amp;ge;98%</td><td>Sigma</td><td>197378</td><td></td></tr><tr><td>Phosphate buffer 1 M</td><td>Sigma</td><td>P3619</td><td></td></tr><tr><td>Propylene oxide (C&lt;sub&gt;3&lt;/sub&gt;H&lt;sub&gt;6&lt;/sub&gt;O), 99%</td><td>Alfa Aesar&amp;nbsp;</td><td>30765</td><td></td></tr><tr><td>Sodium tetrahydroborate</td><td>VWR</td><td>27885.134</td><td></td></tr><tr><td>Sucrose</td><td>Fisher scientific</td><td>S/8600/53</td><td></td></tr><tr><td>Trizma Hydrochloride, &amp;ge;99.0%</td><td>Sigma</td><td>T5941</td><td></td></tr><tr><td>Trizma base, &amp;ge;99.9%</td><td>Sigma</td><td>T6066</td><td></td></tr><tr><td>Vectashield Antifade Mounting Medium, , refractive index 1.45&amp;nbsp;</td><td>Vector laboratories</td><td>H-1000</td><td></td></tr><tr><td>Vectastain Elite ABC HRP kit</td><td>Vector laboratories</td><td>PK6100</td><td></td></tr><tr><td>Equipment used&amp;nbsp;</td><td></td><td></td><td></td></tr><tr><td>Vibratome</td><td>Agar Scientific</td><td></td><td></td></tr><tr><td>C4A Cupped aluminium planchettes&amp;nbsp;</td><td>GA-MA &amp;amp; ASSOCIATES, INC.</td><td></td><td></td></tr><tr><td>Leica DMR microscope&amp;nbsp;</td><td>Leica Microsystems</td><td></td><td></td></tr><tr><td>X-Cite 120PC Q&amp;nbsp; fluorescence light source&amp;nbsp;</td><td>Excelitas Technologies&amp;nbsp;</td><td></td><td></td></tr><tr><td>Leica DFC450 digital microscope camera&amp;nbsp;</td><td>Leica Microsystems&amp;nbsp;</td><td></td><td></td></tr><tr><td>Rapidograph technical drawing pen 0.18mm&amp;nbsp;</td><td>London graphics centre</td><td></td><td></td></tr><tr><td>0.18 mm rapidograph nib</td><td>London graphics centre</td><td></td><td></td></tr><tr><td>Rapidograph technical drawing pen 0.25mm&amp;nbsp;</td><td>London graphics centre</td><td></td><td></td></tr><tr><td>0.25 mm rapidograph nib</td><td>London graphics centre</td><td></td><td></td></tr><tr><td>Neurolucida system including PC workstation, stage, camera and joystic for XYZ stage control</td><td>Microbrighfield (MBF) Bioscience</td><td></td><td></td></tr><tr><td>Neurolucida software version 2017</td><td>Microbrighfield (MBF) Bioscience</td><td></td><td></td></tr><tr><td>CorelDRAW graphics Suite X5</td><td>Corel</td><td></td><td></td></tr><tr><td>Video editing software&amp;nbsp;</td><td>Adobe Premiere Pro</td><td></td><td></td></tr><tr><td>Glass vials 14 mL</td><td>Fisher scientific&amp;nbsp;</td><td></td><td></td></tr></tbody></table>

biocytin recovery and 3d reconstructions of filled hippocampal ca2 interneurons

How cortical network activity processes information is of importance to a large number of basic and clinical scientific questions. The protocol described here identifies the basic building blocks of this circuitry. The in-depth studies of cortical regions will ultimately provide other scientists with the circuit components needed for an understanding of how the brain acquires, processes and stores information and what goes wrong in disease, while the electrophysiological and morphological data are widely used by computational neuroscientists in the construction of model networks that explore information processing. The protocol outlined here describes how biocytin-filled cells recorded in the CA2 region of the hippocampus are recovered and then reconstructed in&#160;3D. Additionally, the protocol describes the demonstration of calcium binding protein or peptide content in recorded interneurons.

Neurons in hippocampal CA2 were filled with biocytin following electrophysiological recordings (Figures 1Ac, Ad and 1Bc, Bd). The slices were fixed overnight following the recordings and the neurochemistry and morphological characterization of neurons were revealed following the protocol described here.
The calcium binding protein or protein content of filled interneurons was determined by incubating the slices first with primary antibodies and then with fluorescently labelled secondary antibodies. The firing characteristics of the interneurons during the recordings will dictate the choice of primary antibodies used. Avidin-AMCA was used to visualize the biocytin-filled interneuron and anti-mouse fluorescein isothiocyanate (FITC) and goat anti-rabbit Texas Red (TR) were used to characterize the interneuronal neurochemistry (Figure 1Bb).
Following the fluorescence visualization, an HRP protocol was used to reveal the biocytin (Figure 1Ab). The fine detailed anatomy of CA2 interneurons was then drawn in 3D using a neuron reconstruction software (Figure 2 and Figure 3a). A video of a 3D reconstruction of a basket cell recorded and filled in CA2 is displayed in Video. Neuronal reconstructions were considered as complete if both the dendritic and axonal arbors were confined within the depth of the 450-500 &#956;m slice. Poor axonal arbor staining was assessed by the presence of truncated branches with open endings at the top or the bottom of the slice or by a staining that was limited to the axon initial segment and very proximal branches. Figure 4 represents the examples of a good and a poor HRP staining following biocytin visualization.
Morphometric analysis of 3D reconstructions (Figure 3) can be carried out to demonstrate branch complexity, soma surface area and the surface area and volume of the dendritic and axonal arbors.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/58592/58592fig1.jpg" /> 
Figure 1:&#160;Neuronal reconstructions of two types of basket cells recorded and filled in the hippocampal CA2 region and correlated electrophysiological data obtained following intracellular recordings in vitro. This figure has been modified from previous studies23,24. SO Stratum Oriens, SP Stratum Pyramidale, SR Stratum Radiatum, SLM Stratum Lacunosum Moleculare. (A) Aa: Reconstruction of a CA2 basket cell with restricted dendritic and axonal arbor using a drawing tube (1000X). The dendrites are in black, and the axon is in red. Ab: Image of the biocytin-filled basket cell following the avidin-HRP protocol described here. Ac: Representative trace of voltage responses to hyperpolarizing and depolarizing current injection of a CA2 basket cell with restricted dendritic and axonal arbor. Ad: Example of a CA2 pyramid to narrow arbor basket cell connections recorded using sharp electrodes. Composite excitatory post-synaptic potential (EPSP) averages show brief train depression apparent during responses to trains of three spikes. (B) Ba: 2D reconstruction of a CA2 basket cell with wide dendritic and axonal arbors using a drawing tube (1000X). The dendritic tree of this basket cell (in black) extended radially through all layers of the CA2 region and horizontally in SO and SP of the CA2 and CA3 regions. One horizontal dendrite also reached the CA1 region. The axon (in red) extended to the CA3 and CA1 regions. Bb: The biocytin-filled (AMCA staining) basket cell was PV-immunopositive (FITC staining) and CB-immunonegative (Texas-Red staining). Bc: Representative trace of voltage responses to hyperpolarizing and depolarizing current injection of a CA2 basket cell with wide dendritic and axonal arbor. Bd: Composite EPSP averages show brief train facilitation apparent during responses to trains of three spikes. Examples of other types of interneurons recorded in CA2 can be found in previous studies25,30. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/58592/58592fig1large.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/58592/58592fig2.jpg" /> 
Figure 2:&#160;3D cell body reconstruction. (A) 3D tracing of the cell body. View of the different contours traced at different z positions whilst focusing through the cell body. (B) 3D view of the different contours. (C) 3D view of the cell body at a different angle. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/58592/58592fig2large.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/58592/58592fig3.jpg" /> 
Figure 3:&#160;Morphometry analyses of 3D neuronal reconstructions. (A) 3D reconstruction of a CA2 narrow arbor basket cell. Each dendritic branch is represented by a color (green, blue, red and pink) and axon is in light blue. (B) Dendrogram of the basket cell representing the number of dendritic branches and length of each segment contained within spheres concentric with the soma and at 100 &#956;m intervals from the soma. The colors on the dendrogram correspond to those of the dendrites in A. (C) Example of morphometric analysis performed on CA2 pyramidal cells (adapted from a previous study23). The number of dendritic branches was plotted against the distance from the soma of CA2 pyramidal cells. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/58592/58592fig3large.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/58592/58592fig4.jpg" /> 
Figure 4:&#160;Examples of good (A) and poor (B) HRP staining. (A) Biocytin recovery revealed a very well filled interneuron in CA2. The cell body (CB) is darkly stained and has clear outlines. The dendrites are beaded and displayed some spines (represented by red stars). The axonal arbor (A) is dense and presents small boutons. (B) Example of a poor dendritic and axonal staining of 2 pyramidal cells in CA2. The staining of the CB is faint with no clear outline. Poor staining is often associated with shorter electrophysiological recordings resulting in the presence of very few biocytin-filled branches. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/58592/58592fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
Video 1:&#160;3D neuronal reconstruction of a CA2 basket cell with restricted dendritic arbor (also referred to as CA2 narrow arbor basket cell) with its soma in stratum pyramidale, dendrites spanning all layers and axon in CA2 stratum pyramidale and adjacent stratum oriens and radiatum. Very few branches reached the proximal CA3 stratum oriens and CA3 stratum pyramidale. This cell was filled with biocytin following electrophysiological recordings and sections were processed with avidin-HRP following the protocol described here. Due to slicing, only the axon within the depth of the slice was recovered, though the dendrites are intact. Dendrites are in dark pink and axon in white. Layer and region boundaries have been added at the beginning of the video. 3D reconstruction by Georgia Economides- 3D video by Svenja Falk. The video was recorded with a neuron reconstruction software as stated in Step 2.17 and edited with a video editing software. Link to the video:30.&#160;<a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/58592/Figure_3.mp4" target="_blank">Please click here to download this video.</a>

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Solutions used&#160;</td>
			<td>Composition/Instructions</td>
		</tr>
		<tr>
			<td>Fixation solution</td>
			<td>4% paraformaldehyde, 0.2% saturated picric acid solution, 0.025% glutaraldehyde solution in 0.1 M phosphate buffer (PB)</td>
		</tr>
		<tr>
			<td>0.1M Phosphate Buffer pH 7.6</td>
			<td>Add 100 mL of stock 1 M Phosphate Buffer to 900 mL of distilled water&#160;</td>
		</tr>
		<tr>
			<td>Phosphate buffered saline (PBS) pH 7.4/7.5</td>
			<td>Add 10 mL of 0.1M phosphate buffer, 0.2 g of KCl and 8.76 g of NaCl to 990 mL of distilled water</td>
		</tr>
		<tr>
			<td>TRIS buffer pH 7.5</td>
			<td>Dissolve 5.72 g of Tris Hydrochloride and 1.66 g of Tris Base in 50 mL of distilled water. Then make up to 1 L with distilled water.</td>
		</tr>
		<tr>
			<td>Buffered glutaraldehyde and paraformaldehyde fixative solution</td>
			<td>4% paraformaldehyde, 0.2% saturated picric acid solution, 0.025% glutaraldehyde solution in 0.1 M Phosphate buffer.&#160;</td>
		</tr>
		<tr>
			<td>ABC solution&#160;</td>
			<td>Solution to be made at least 30 min before use from the ABC kit. Add 1 drop of solution A and 1 drop of solution B to 2.5 mL of PBS.</td>
		</tr>
		<tr>
			<td>Durcupan epoxy resin:&#160;</td>
			<td>To make 20 pots: 20 g of component A, 20 g of component B, 0.6 g of component C and 0.4 g of component D-&#160;</td>
		</tr>
		<tr>
			<td></td>
			<td>Protect the balance from spills by covering the plate with a circle of filter paper. Carefully weigh the reagents into a tripour beaker in the proportions stated above. Mix thoroughly by vigorously stirring using two wooden sticks for at least 5 min. The mixture should become a uniform density dark brown colour. Place the beaker into the oven at ~50 &#176;C for a maximum of 10 min to remove as many air bubbles as possible. NOTE: The resin will start to cure if you leave the beaker in the oven longer than 10 min. Decant the resin out into plastic pots or 5 mL syringes, date them and store in the -20 &#176;C freezer ready for use.</td>
		</tr>
	</tbody>
</table>
Table 1: Table of solutions.&#160;

Watch this Scientific Journal Video about Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons at JoVE.com

Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons

The protocol outlined here describes the immunofluorescence analysis, biocytin recovery and high-quality reconstructions of hippocampal CA2 interneurons following the intracellular electrophysiological recordings in vitro, allowing neuronal characterization and ultimately fine neuronal anatomy to be studied.

How cortical network activity processes information is of importance to a large number of basic and clinical scientific questions. The protocol described ...

biocytin-recovery-3d-reconstructions-filled-hippocampal-ca2

Research

JoVE Journal

Neuroscience

8.4K Views.  University College London. Deze methode kan helpen bij het classificeren van neuronale subtypes en ons begrip van de functionele kaart van corticale circuits uit te breiden. Dit protocol is geoptimaliseerd om de ultrastructuur van de neuronen te behouden en een uitstekend herstel van zowel dendritische als axonale prieel arbors te verkrijgen, waardoor reconstructies van hoge kwaliteit mogelijk zijn. Breng aan het einde van een elektrofysiologische opname het segment met de opgenomen cel over naar een klein gerecht van ...

Video: Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons

Studying Protein Function and the Role of Altered Protein Expression by Antibody Interference and Three-dimensional Reconstructions

A strict management of protein expression is not only essential to every organism alive, but also an important strategy to investigate protein functions in cellular models. Therefore, recent research invented different tools to target protein expression in mammalian cell lines or even animal models, including RNA and antibody interference. While the first strategy has gathered much attention during the past two decades, peptides &#160;mediating a translocation of antibody cargos across cellular membranes and into cells, obtained much less interest. In this publication, we provide a detailed protocol how to utilize a peptide carrier named Chariot in human embryonic kidney cells as well as in primary hippocampal neurons to perform antibody interference experiments and further illustrate the application of three-dimensional reconstructions in analyzing protein function. Our findings suggest that Chariot is, probably due to its nuclear localization signal, particularly well-suited to target proteins residing in the soma and the nucleus. Remarkably, when applying Chariot to primary hippocampal cultures, the reagent turned out to be surprisingly well accepted by dissociated neurons.

Controlling protein expression is not only essential to every organism alive, but also an important strategy to investigate protein functions in cellular models. The protocol presented shows the application of antibody interference in mammalian cells including primary hippocampal neurons and demonstrates the use of three-dimensional reconstructions in studying protein function.

A strict management of protein expression is not only essential to every organism alive, but also an important strategy to investigate protein functions ...

Bioengineering

Juxtasomal Biocytin Labeling to Study the Structure-function Relationship of Individual Cortical Neurons

The cerebral cortex is characterized by multiple layers and many distinct cell-types that together as a network are responsible for many higher cognitive functions including decision making, sensory-guided behavior or memory. To understand how such intricate neuronal networks perform such tasks, a crucial step is to determine the function (or electrical activity) of individual cell types within the network, preferentially when the animal is performing a relevant cognitive task. Additionally, it is equally important to determine the anatomical structure of the network and the morphological architecture of the individual neurons to allow reverse engineering the cortical network. Technical breakthroughs available today allow recording cellular activity in awake, behaving animals with the valuable option of post&#160;hoc identifying the recorded neurons. Here, we demonstrate the juxtasomal biocytin labeling technique, which involves recording action potential spiking in the extracellular (or loose-patch) configuration using conventional patch pipettes. The juxtasomal recording configuration is relatively stable and applicable across behavioral conditions, including anesthetized, sedated, awake head-fixed, and even in the freely moving animal. Thus, this method allows linking cell-type specific action potential spiking during animal behavior to reconstruction of the individual neurons and ultimately, the entire cortical microcircuit. In this video manuscript, we show how individual neurons in the juxtasomal configuration can be labeled with biocytin in the urethane-anaesthetized rat for post&#160;hoc identification and morphological reconstruction.

To understand the structure of neuronal networks, functional and morphological characterization of individual neurons is a necessity. Here, we demonstrate juxtasomal biocytin labeling, which allows electrophysiological recordings in the extracellular configuration, yet maintaining the ability to intracellularly label the neuron for post&#160;hoc reconstruction of dendritic and axonal architecture.

The cerebral cortex is characterized by multiple layers and many distinct cell-types that together as a network are responsible for many higher cognitive ...

Whole-cell Patch-clamp Recordings from Morphologically- and Neurochemically-identified Hippocampal Interneurons

GABAergic inhibitory interneurons play a central role within neuronal circuits of the brain. Interneurons comprise a small subset of the neuronal population (10-20%), but show a high level of physiological, morphological, and neurochemical heterogeneity, reflecting their diverse functions. Therefore, investigation of interneurons provides important insights into the organization principles and function of neuronal circuits. This, however, requires an integrated physiological and neuroanatomical approach for the selection and identification of individual interneuron types. Whole-cell patch-clamp recording from acute brain slices of transgenic animals, expressing fluorescent proteins under the promoters of interneuron-specific markers, provides an efficient method to target and electrophysiologically characterize intrinsic and synaptic properties of specific interneuron types. Combined with intracellular dye labeling, this approach can be extended with post-hoc morphological and immunocytochemical analysis, enabling systematic identification of recorded neurons. These methods can be tailored to suit a broad range of scientific questions regarding functional properties of diverse types of cortical neurons.

Cortical networks are controlled by a small, but diverse set of inhibitory interneurons. Functional investigation of interneurons therefore requires targeted recording and rigorous identification. Described here is a combined approach involving whole-cell recordings from single or synaptically-coupled pairs of neurons with intracellular labeling, post-hoc morphological and immunocytochemical analysis.

GABAergic inhibitory interneurons play a central role within neuronal circuits of the brain. Interneurons comprise a small subset of the neuronal ...

Electrophysiological and Morphological Characterization of Neuronal Microcircuits in Acute Brain Slices Using Paired Patch-Clamp Recordings

The combination of patch clamp recordings from two (or more) synaptically coupled neurons (paired recordings) in acute brain slice preparations with simultaneous intracellular biocytin filling allows a correlated analysis of their structural and functional properties. With this method it is possible to identify and characterize both pre- and postsynaptic neurons by their morphology and electrophysiological response pattern. Paired recordings allow studying the connectivity patterns between these neurons as well as the properties of both chemical and electrical synaptic transmission. Here, we give a step-by-step description of the procedures required to obtain reliable paired recordings together with an optimal recovery of the neuron morphology. We will describe how pairs of neurons connected via chemical synapses or gap junctions are identified in brain slice preparations. We will outline how neurons are reconstructed to obtain their 3D morphology of the dendritic and axonal domain and how synaptic contacts are identified and localized. We will also discuss the caveats and limitations of the paired recording technique, in particular those associated with dendritic and axonal truncations during the preparation of brain slices because these strongly affect connectivity estimates. However, because of the versatility of the paired recording approach it will remain a valuable tool in characterizing different aspects of synaptic transmission at identified neuronal microcircuits in the brain.

Patch-clamp recordings and simultaneous intracellular biocytin filling of synaptically coupled neurons in acute brain slices allow a correlated analysis of their structural and functional properties. The aim of this protocol is to describe the essential technical steps of electrophysiological recording from neuronal microcircuits and their subsequent morphological analysis.

The combination of patch clamp recordings from two (or more) synaptically coupled neurons (paired recordings) in acute brain slice preparations with ...

Immunostaining of Biocytin-filled and Processed Sections for Neurochemical Markers

Electrophysiological recordings of cells using the patch clamp technique have allowed for the identification of different neuronal types based on firing patterns. The inclusion of biocytin/neurobiotin in the recording electrode permits post-hoc recovery of morphological details, which are necessary to determine the dendritic arborization and the regions targeted by the axons of the recorded neurons. However, given the presence of morphologically similar neurons with distinct neurochemical identities and functions, immunohistochemical staining for cell-type-specific proteins is essential to definitively identify neurons. To maintain network connectivity, brain sections for physiological recordings are prepared at a thickness of 300 &#181;m or greater. However, this thickness often hinders immunohistological postprocessing due to issues with antibody penetration, necessitating the resectioning of the tissue. Resectioning of slices is a challenging art, often resulting in the loss of tissue and morphology of the cells from which electrophysiological data was obtained, rendering the data unusable. Since recovery of morphology would limit data loss and guide in the selection of neuronal markers, we have adopted a strategy of recovering cell morphology first, followed by secondary immunostaining. We introduce a practical approach to biocytin filling during physiological recordings and subsequent serial immunostaining for the recovery of morphology, followed by the restaining of sections to determine the neurochemical identity. We report that sections that were filled with biocytin, fixed with paraformaldehyde (PFA), stained, and coverslipped can be removed and restained with a second primary antibody days later. This restaining involves the removal of the coverslip, the washing of sections in a buffer solution, and the incubation of primary and secondary antibodies to reveal the neurochemical identity. The method is advantageous for eliminating data loss due to an inability to recover morphology and for narrowing down the neurochemical markers to be tested based on morphology.

This protocol presents a method for the morphological recovery of neurons patched during electrophysiological recordings using biocytin filling and subsequent immunohistochemical postprocessing. We show that thick biocytin-filled sections that were stained and coverslipped can be restained with a second primary antibody days&#160;or months later.

Electrophysiological recordings of cells using the patch clamp technique have allowed for the identification of different neuronal types based on firing ...

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.

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+ ...

In Vivo Direct Reprogramming of Resident Glial Cells into Interneurons by Intracerebral Injection of Viral Vectors

Converting resident glia in the brain into functional and subtype-specific neurons in vivo provides a step forward towards the development of alternative cell replacement therapies while also creating tools to study cell fate in situ. To date, it has been possible to obtain neurons via in vivo reprogramming, but the precise phenotype of these neurons or how they mature has not been analyzed in detail. In this protocol, we describe a more efficient conversion and cell-specific identification of the in vivo reprogrammed neurons, using an AAV-based viral vector system. We also provide a protocol for functional assessment of the reprogrammed cells&#8217; neuronal maturation. By injecting flip-excision (FLEX) vectors, containing the reprogramming and synapsin-driven reporter genes&#160;to specific cell types in the brain that serve as the target for cell reprogramming. This technique allows for the easy identification of newly reprogrammed neurons. Results show that the obtained reprogrammed neurons functionally mature over time, receive synaptic contacts and show electrophysiological properties of different types of interneurons. Using the transcription factors Ascl1, Lmx1a and Nurr1, the majority of the reprogrammed cells have properties of fast-spiking, parvalbumin-containing interneurons.

This protocol aims at generating directly reprogrammed interneurons in vivo, using an AAV-based viral system in the brain and a FLEX synapsin-driven GFP reporter, which allows for cell identification and further analysis in vivo.

Converting resident glia in the brain into functional and subtype-specific neurons in vivo provides a step forward towards the development of alternative ...

Preparation of Acute Slices from Dorsal Hippocampus for Whole-Cell Recording and Neuronal Reconstruction in the Dentate Gyrus of Adult Mice

Although the general architecture of the hippocampus is similar along its longitudinal axis, recent studies have revealed prominent differences in molecular, anatomical and functional criteria suggesting a division into different sub-circuits along its rostro-caudal extent. Owing to differential connectivity and function the most fundamental distinction is made between the dorsal and the ventral hippocampus, which are preferentially involved in spatial and emotional processing, respectively. Accordingly, in vivo work regarding spatial memory formation has focused on the dorsal hippocampus.
In contrast, electro-physiological in vitro recordings have been preferentially performed on intermediate-ventral hippocampus, largely motivated by factors like slice viability and circuit integrity. To allow for direct correlation of in vivo data on spatial processing with in vitro data we have adapted previous sectioning methods to obtain highly viable transverse brain slices from the dorsal-intermediate hippocampus for long-term recordings of principal cells and interneurons in the dentate gyrus. As spatial behavior is routinely analyzed in adult mice, we have combined this transversal slicing procedure with the use of protective solutions to enhance viability of brain tissue from mature animals. We use this approach for mice of about 3 months of age. The method offers a good alternative to the coronal preparation which is frequently used for in vitro studies on dorsal hippocampus. We compare these two preparations in terms of quality of recordings and preservation of morphological features of recorded neurons.

We present a protocol to prepare acute-slices from the dorsal-intermediate hippocampus of mice. We compare this transversal preparation with coronal slicing in terms of quality of recordings and preservation of morphological features of recorded neurons.

Although the general architecture of the hippocampus is similar along its longitudinal axis, recent studies have revealed prominent differences in ...

Immunostaining of Interneurons in a Rat Hippocampal Section

Swietek, B., et al., <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/54880">Immunostaining of Biocytin-filled and Processed Sections for Neurochemical Markers.</a> J. Vis. Exp. (2016)
This video demonstrates the process of visualizing a biocytin-filled interneuron in a rat hippocampal section, highlighting its neurochemical identity through the use of specific antibodies and fluorescence microscopy.

Swietek, B., et al., Immunostaining of Biocytin-filled and Processed Sections for Neurochemical Markers. J. Vis. Exp. (2016)
This video demonstrates the ...

JoVE Encyclopedia of Experiments

Neuropathology

Neurodegenerative Diseases

Labeling of Biocytin-Filled Interneurons in Rat Hippocampal Slices for Visualization

Source: Economides, G., et al. <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/58592">Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons.</a> J. Vis. Exp. (2018)
This video demonstrates the procedure for staining fixed rat brain slices containing biocytin-filled interneurons. The protocol includes incubation with avidin-biotin complex (ABC), staining with HRP and chromogenic substrate, preserving structures with osmium tetroxide, and embedding the tissue in resin for imaging.

Biocytin Recovery and 3D Reconstructions of Filled Hippocampal CA2 Interneurons

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