C.M.L. acknowledges support of this work by the Air Force Office of Scientific Research (FA9550-14-1-0136), a Harvard University Physical Sciences and Engineering Accelerator award, and a National Institutes of Health Director&#39;s Pioneer Award (1DP1EB025835-01). T.G.S. acknowledges support by the Department of Defense (DoD) through the National Defense Science &#38; Engineering Graduate Fellowship (NDSEG) program. G.H. acknowledges fellowship support from the American Heart Association (16POST27250219) and the Pathway to Independence Award (Parent K99/R00) from the National Institute on Aging of the National Institutes of Health. This work was performed in part at the Harvard University Center for Nanoscale Systems (CNS), a member of the National Nanotechnology Coordinated Infrastructure Network (NNCI), which is supported by the National Science Foundation under NSF ECCS Award No. 1541959.

<ol>
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The authors have nothing to disclose.

All steps in the fabrication and the use of mesh electronics are important, but a few are especially critical. Before releasing the mesh electronics from their wafer, it is essential to oxidize the surface to make the meshes readily suspended in aqueous solution (step 1.6.1). If this step is skipped, the meshes usually float on the surface of the water, making them difficult to load into the needles, and if they can be loaded, they often stick to the sides of the glass needles, requiring large volumes (&#62;100 &#181;L) for the injection. Failure to oxidize the surface before release, therefore, typically means that the meshes cannot be used and the fabrication must be re-performed from the beginning. Another critical step is bending the mesh electronics &#34;stem&#34; to ~90&#176; during the I/O interfacing (step 4.3). If the angle is less than 90&#176;, then all 32 I/O pads will not fit into the ZIF connector; some will have to be cut off the end to allow the insertion, reducing the number of connected electrodes. The process must also be done gently to prevent the stem from breaking.
The design of mesh electronics can be customized for various applications by modifying the photomasks and using the same fabrication procedure outlined in Figure 2. For example, while the mesh electronics probes used to record the data in Figure 9 were designed to have 32 recording electrodes span the mouse hippocampus and primary somatosensory cortex, the electrode placement within the ultraflexible mesh can be selected to target virtually any brain region(s), or larger electrodes for stimulation can be incorporated27. The same basic mesh structure and fabrication procedure are retained, but the electrode placement and design are adjusted to meet the needs of the study. Investigators should use caution, however, and always test that modified designs can be injected easily through the intended needles. Small changes to the bending mechanics of mesh electronics can have substantial effects on injectability. One such example is that a 45&#176; angle between transverse and longitudinal SU-8 ribbons yields a mesh electronics probe that can be facilely injected but a 90&#176; angle results in one that crumples and clogs needles21.
Measuring the impedance of the recording electrodes is helpful for troubleshooting. A 20-&#181;m diameter circular Pt electrode should have an impedance magnitude near 1 M&#937; when measured at a frequency of 1 kHz in vivo or in 1x PBS29. An impedance significantly larger than this implies that the electrode is not exposed, as may happen if it is contaminated with photoresist residue, or not electrically connected. The latter may occur if, for example, there is dust on the photo mask during PL that results in a disconnect in the Au interconnects, or if one of the mesh I/O pads is not contacted by the ZIF connector pins during I/O interfacing. An impedance magnitude roughly half the expected value suggests that the channel may be shorted to the adjacent one, creating a circuit of two electrode impedances in parallel to each other. The measured impedance values act as a guide during troubleshooting; combined with optical microscopy of the mesh electronics probes, the source of the problem can usually be identified and corrected accordingly in the next fabrication run or I/O interfacing attempt.
The use of syringe-injectable mesh electronics for acute studies is limited in that single-unit spiking activity usually is not observed until 1 week post injection27, although recent work (unpublished) shows that this issue is readily overcome. Key determinants of the time required to see spiking activity are the mesh design, the volume of fluid injected into the brain along with mesh electronics, and the diameter of the needle used for injection, as these affect the degree of tissue damage during the injection and the rate of healing. Large injection volumes may be required if the mesh electronics are not treated with oxygen plasma prior to the release in Ni etchant; that is, if the mesh is not hydrophilic, it can adhere to the glass needle. Occasionally, the meshes have defects that lead to bending mechanics which make them difficult to inject. During the loading of the mesh electronics, it is important to check that meshes are moving easily and smoothly within the needle (as shown in Supplementary Video 1). If not, a different mesh electronic probe should be used. Best results for seamless neural interfacing will be achieved with the ideal injection volumes of 10&#8211;50 &#181;L per 4 mm of injected mesh length. More recent results with finer mesh electronics probes injected and/or smaller diameter capillary needles (as small as 150 &#181;m inner diameter, 250 &#181;m outer diameter) show that single unit spiking can be observed from shortly after the injection (acute measurements) through longer times. Mask design files for these finer mesh structures are available by request or from the resource website, meshelectronics.org. We estimate the overall yield of our in vivo mesh injection procedures using 400 &#181;m inner diameter (650 &#181;m outer diameter) needles to be around 70%, although the yield is closer to 80&#8211;90% for our more recent work with 150 &#181;m inner diameter (250 &#181;m outer diameter) needles. The most common reasons for failure are (1) that the mesh does not inject smoothly, resulting in brain edema from unexpectedly large injection volumes into the brain, (2) mesh breakage during the manual manipulation required in the I/O interfacing procedure, and (3) bleeding from damaging a blood vessel during injection. Damaging a blood vessel during injection is rare (the cause of less than 10% of failures) and could be reduced further by using image-guided surgery. We also note that damage of blood vessels is a common limitation of all procedures involving penetration of the brain tissue, including injection of viral particles for transfection, implantation of rigid brain probes, and injection of the mesh electronics.
Mesh electronics probes are able to stably record from and track the same individual neurons on at least months to year timescales and evoke almost no chronic immune response, as demonstrated in Figure 9 and Figure 10, respectively. This represents a significant advantage compared to convention depth electrodes, which commonly suffer from decreasing spike amplitudes, unstable signals, and chronic inflammation over the course of long-term recording experiments14,15. Additionally, the mesh electronics have the advantage that they can be left in the tissue during histological sectioning, staining, and imaging, in contrast to conventional probes, which are too rigid and must therefore be removed prior to histology analyses. Hence, mesh electronics allow for the unique ability to use immunohistochemical analysis to precisely study the cellular environment surrounding each recording site.
The protocol presented here opens-up exciting new opportunities in neuroscience. The minimally invasive delivery method and seamless integration of mesh electronics with brain tissue minimizes disruption to neural circuits and avoids chronic immune response, which could benefit most types of chronic neural recording experiments. The ability of mesh electronics to record and track the same single neurons for long periods of time will especially be of interest to investigators seeking to correlate millisecond-scale spiking activity with month- to year-long processes such as aging, the pathogenesis of brain disease, or brain development16,18. Additionally, there exist substantial opportunities to extend and customize this protocol, such as adding active electronics to the PCB head-stage to implement functionality like digital multiplexing8,35, wireless communication35,36,37, and signal processing35, co-injecting stem cells or polymers with the mesh electronics to aid in tissue regeneration18,38,39, and incorporating nanowire field-effect transistors (NW-FETs) into mesh electronics for highly localized and multifunctional brain probes24,29,40,41,42.

The development of tools capable of mapping the brain with single-neuron resolution is of central importance to neuroscience and neurology. Noninvasive technologies for neural studies such as electroencephalography (EEG), magnetoencephalography (MEG), and functional magnetic resonance imaging (fMRI) have proven valuable for correlating brain activity with behavior in humans1,2, but they lack the spatiotemporal resolution necessary for studying the structure and dynamics of neural networks at their fundamental micrometer and millisecond scales, respectively3,4. Certain electrocorticography (ECoG) probes and optical imaging methods using voltage-sensitive dyes have succeeded in recording single-unit spiking activity in vivo5,6, but they are generally effective only near the brain surface, limiting&#160;applicability to&#160;studies of shallow brain regions. In contrast, implantable electrical probes can measure single-neuron electrophysiology in freely moving animals from virtually any brain region without the need for fluorescent labeling, making them indispensable to systems-level neuroscience, especially as microfabrication techniques from the semiconductor industry have pushed channel counts into the hundreds and thousands3,7,8,9. By virtue of these capabilities, implantable electrical probes have made many important contributions to neuroscience and neurology, including fundamental studies of information processing in the visual system10, the treatment of neurological disorders such as Parkinson&#39;s disease11, and the demonstration of brain-machine interfaces (BMIs) for advanced prosthetics12,13.
Nevertheless, long-term instability manifested as decreasing spike amplitudes and unstable signals on timescales of weeks to months14,15 has limited the applicability of implantable probes to the study of relatively short-term phenomena, leaving questions such as brain aging and development largely unanswered. The limitations in long-term instability are a result of a mismatch between conventional probes and brain tissue in size, mechanics, and topology14,15,16,17,18. In terms of size, while neuronal synapses and somata are approximately tens of nanometers to tens of micrometers in diameter19, respectively, traditional probes are often significantly larger, in the case of silicon microelectrode arrays &#62;4 times the size of a single neuron cell body7,8. The relatively large size of these probes may disrupt the natural structure and connectivity of dense neural tissue, thus contributing to chronic immune response and perturbing the neural circuitry being studied. In terms of mechanical properties, traditional probes are drastically stiffer than the extremely soft neural tissue in which they are implanted; even &#34;flexible&#34; probes made from 10&#8211;20 &#181;m thick sheets of polyimide are at least 100,000 times stiffer than brain tissue20,21. This mismatch in bending stiffness causes relative shear motion between the probe and brain tissue, leading to unreliable single-unit tracking during extended recordings and inducing chronic gliosis at the implantation site. Finally, the topological structure of conventional brain probes necessarily excludes a solid volume of the tissue. Such mismatch in topology disrupts the connectivity of neural circuits, precludes the natural three-dimensional (3D) interpenetrated distribution of neurons, glial cells, and blood vessels within brain tissue22, and hinders 3D transport of signaling molecules23. Together, these shortcomings of conventional probes have made them fall short of the long-term compatibility sought for clinical applications and longitudinal neuroscience studies at the single-neuron level.
To overcome these shortcomings, we sought to blur the line between the neural and electronic systems by developing a new paradigm of &#34;tissue-like&#34; neural probes termed mesh electronics16,21,24. Mesh electronics addresses the above matching issues in size, mechanics, and topology by incorporating (1) structural features of the same nanometer to micrometer size scale of neural tissue, (2) mechanical properties similar to those of brain tissue, and (3) a 3D macroporous topology that is &#62;90% open space and thus accommodates interpenetration by neurons and diffusion of molecules through the extracellular environment. Mesh electronics probes can be precisely delivered to specific brain regions through a syringe and a needle, causing minimal acute damage while implanting even in deep brain regions21,25. Neuronal soma and axons have been shown to interpenetrate the open 3D mesh electronics probe structure within weeks post-injection, thereby creating a seamless, gliosis-free interface between recording electronics and surrounding brain tissue21,26,27. These unique features have enabled mesh electronics probes to stably track spiking activity from the same individual neurons over at least a year timescale27. Moreover, the fabrication of the mesh electronics based on photolithography (PL) provides high scalability of the number of electrodes that can be incorporated, with demonstrated channel counts up to 128 electrodes per probe using simple contact mask lithography28 and a plug-and-play input/output (I/O) design that allows for rapid electrical connection to peripheral electronics without specialized equipment29.
A broad range of studies may benefit from incorporating mesh electronics into measurement protocols. Most intracortical recording experiments could benefit from mesh electronics&#39; minimally invasive implantation procedure via syringe injection, the drastically reduced immune response following implantation, and the ability to leave mesh electronics in the tissue during subsequent histology and immunostaining for precise analysis of the biological environment surrounding each recording site. Chronic recording experiments in particular will derive value from the unique ability of mesh electronics to track large numbers of individual neurons for months to years. This capability creates opportunities for studies with single-neuron resolution that were previously impractical, such as longitudinal aging studies of neural circuits, investigations of the developing brain, and inquiries into the pathogenesis of encephalopathies16.
In this protocol, we describe all the key steps in a typical mouse neural recording experiment using syringe-injectable mesh electronics (see Figure 1). Steps described include the fabrication of mesh electronics in a standard PL-based process possible at many universities, loading mesh electronics into standard capillary needles, stereotaxic injection of mesh electronics in vivo, connection of the mesh I/O to standard instrumentation interfaces, restrained or freely moving recording sessions, and histological sectioning of brain tissue containing mesh electronics. Some researchers using mesh electronics only for histology studies may not require electrical interfacing and recording, in which case they may skip those steps. After familiarizing themselves with this protocol, investigators should have all the knowledge necessary to use mesh electronics in their own experiments.

<table><tbody><tr><td>Motorized stereotaxic frame</td><td>World Precision Instruments</td><td>MTM-3</td><td>For mouse stereotaxic surgery</td></tr><tr><td>512-channel recording controller</td><td>Intan Technologies</td><td>C3004</td><td>A component of the neural recording system</td></tr><tr><td>RHD2132 amplifier board</td><td>Intan Technologies</td><td>C3314</td><td>A component of the neural recording system</td></tr><tr><td>RHD2000 3 feet ultra thin SPI interface cable</td><td>Intan Technologies</td><td>C3213</td><td>A component of the neural recording system</td></tr><tr><td>Mouse restrainer</td><td>Braintree Scientific</td><td>TV-150&amp;nbsp;STD</td><td>Standard 1.25 inch inner diameter; used to restrain the mouse during restrained recording sessions.</td></tr><tr><td>Si wafers</td><td>Nova Electronic Materials</td><td></td><td>3&quot; P &amp;lt;100&gt; .001-.005 ohm-cm 356-406 &amp;mu;m Thick&lt;br/&gt; Prime Grade SSP Si wafers w/2 Semi-Std. Flats &amp;amp;&lt;br/&gt; 6,000 A&amp;deg;&amp;plusmn;5% Wet Thermal Oxide on both sides.</td></tr><tr><td>Photomasks (chrome on soda lime glass)</td><td>Advance Reproductions</td><td></td><td>Advance Reproductions and other vendors manufacture photomasks from provided design files. Our photomask design files are available by request or from the resource website, meshelectronics.org. Alternatively, some university clean rooms have mask writers for making photomasks on site.</td></tr><tr><td>AutoCAD software</td><td>Autodesk Inc.</td><td></td><td>Design software for drawing photomasks. A free alternative is LayoutEditor. Our photomask design files are available by request or from the resource website, meshelectronics.org.</td></tr><tr><td>Thermal evaporator</td><td>Sharon Vacuum</td><td></td><td>Used to evaporate Ni, Cr, and Au onto mesh electronics during fabrication. Many university clean rooms have this or a similar tool.</td></tr><tr><td>SU-8 2000.5 negative photoresist</td><td>MicroChem Corp.</td><td></td><td>Negative photoresist used to define the bottom and top passivating layers of mesh electronics.</td></tr><tr><td>MA6 mask aligner</td><td>Karl Suss Microtec AG</td><td></td><td>Used to align each photomask to the pattern on the wafer and expose the wafer to UV light. Most university clean rooms have this or a similar tool.</td></tr><tr><td>SU-8 developer</td><td>MicroChem Corp.</td><td></td><td>Used to develop SU-8 negative photoresist following exposure to UV light.</td></tr><tr><td>LOR3A lift-off resist</td><td>MicroChem Corp.</td><td></td><td>Used with Shipley 1805 photoresist to promote undercutting during metal lift-off processes</td></tr><tr><td>Shipley 1805 positive photoresist</td><td>Microposit, The Dow Chemical Company</td><td></td><td>Positive photoresist used to define metal interconnects and Pt electrodes in mesh electronics</td></tr><tr><td>MF-CD-26 positive photoresist developer</td><td>Microposit, The Dow Chemical Company</td><td></td><td>To develop S1805 positive photoresist after exposure in a mask aligner. Many university clean rooms stock this chemical.</td></tr><tr><td>Spin coater</td><td>Reynolds Tech</td><td></td><td>For coating wafers with positive and negative resists. Most university clean rooms have spin coaters.</td></tr><tr><td>PJ plasma surface treatment system</td><td>AST Products, Inc.</td><td></td><td>Used to oxidize the surface of mesh electronics prior to release into aqueous solution. Most university clean rooms have this or a similar tool.</td></tr><tr><td>Electron beam evaporator</td><td>Denton Vacuum</td><td></td><td>For evaporating Cr and Pt during fabrication of mesh electronics. Many university clean rooms have this or a similar tool.</td></tr><tr><td>Remover PG</td><td>MicroChem Corp.</td><td></td><td>Used to dissolve LOR3A and Shipley S1805 resists during metal lift-off</td></tr><tr><td>Ferric chloride solution</td><td>MG Chemicals</td><td>415-1L</td><td>A component of Ni etching solution</td></tr><tr><td>36% hydrochloric acid solution</td><td>Kanto Corp.</td><td></td><td>A component of Ni etching solution</td></tr><tr><td>Glass capillary needles</td><td>Drummond Scientific Co.</td><td></td><td>Inner diameter 0.40 mm, outer diameter 0.65 mm. Other diameters are available.</td></tr><tr><td>Micropipette holder U-type</td><td>Molecular Devices, LLC</td><td>1-HL-U</td><td>Used to hold the glass capillary needles during stereotaxic injection</td></tr><tr><td>1 mL syringe</td><td>NORM-JECT&amp;reg;, Henke Sass Wolf</td><td></td><td>Used for manual loading of mesh electronics into capillary needles</td></tr><tr><td>Polyethylene intrademic catheter tubing</td><td>Becton Dickinson and Company</td><td></td><td>Inner diameter 1.19 mm, outer diameter 1.70 mm</td></tr><tr><td>5 mL syringe</td><td>Becton Dickinson and Company</td><td></td><td>Used in the syringe pump for injection of mesh electronics in vivo</td></tr><tr><td>Eyepiece camera</td><td>Thorlabs Inc.</td><td>DCC1240C</td><td>Used to view mesh electronics within capillary needles during injection</td></tr><tr><td>ThorCam uc480 image acquisition software for USB cameras</td><td>Thorlabs Inc.</td><td></td><td>Used to view mesh electronics within capillary needles during injection</td></tr><tr><td>Syringe pump</td><td>Harvard Apparatus</td><td>PHD 2000</td><td>Used to flow precise volumes of solution through capillary needles during injection of mesh electronics</td></tr><tr><td>EXL-M40 dental drill</td><td>Osada</td><td>3144-830</td><td>For drilling the craniotomy</td></tr><tr><td>0.9 mm drill burr</td><td>Fine Science Tools</td><td>19007-09</td><td>For drilling the craniotomy</td></tr><tr><td>Hot bead sterilizer 14 cm</td><td>Fine Science Tools</td><td>18000-50</td><td>Used to sterlize surgical instruments</td></tr><tr><td>CM1950 cryosectioning instrument</td><td>Leica Microsystems</td><td></td><td>Used to slice frozen tissue into sections. Many universities have this or a similar tool available in a shared facility.</td></tr><tr><td>0.3% Triton x-100</td><td>Life Technologies</td><td></td><td>Used for histology</td></tr><tr><td>5% goat serum</td><td>Life Technologies</td><td></td><td>Used for histology</td></tr><tr><td>3% goat serum</td><td>Life Technologies</td><td></td><td>Used for histology</td></tr><tr><td>Rabbit anti-NeuN</td><td>Abcam</td><td>ab177487</td><td>Used for histology</td></tr><tr><td>Mouse anti-Neurofilament</td><td>Abcam</td><td>ab8135</td><td>Used for histology</td></tr><tr><td>Rat anti-GFAP</td><td>Thermo Fisher Scientific Inc.</td><td>PA516291</td><td>Used for histology</td></tr><tr><td>ProLong Gold Antifade Mountant</td><td>Thermo Fisher Scientific Inc.</td><td>P36930</td><td>Used for histology</td></tr><tr><td>Poly-D-lysine</td><td>Sigma-Aldrich Corp.</td><td>P6407-5MG</td><td>Molecular weight = 70-150 kDA</td></tr><tr><td>Right-angle end clamp</td><td>Thorlabs Inc.</td><td>RA180/M</td><td>Used to attach the pipette holder to the stereotaxic frame</td></tr><tr><td>Printed circuit board (PCB)</td><td>Advanced Circuits</td><td></td><td>Used to interface between mesh electronics and peripheral measurement electronics such as the Intan recording system. Advanced Circuits and other vendors manufacture and assemble PCBs based on provided design files. Our PCB design files are available by request or at the resource site meshelectronics.org</td></tr><tr><td>32-channel standard amplifier connector</td><td>Omnetics Connector Corp.</td><td>A79024-001</td><td>Component assembled onto the PCB</td></tr><tr><td>32-channel flat flexible cable (FFC)</td><td>Molex, LLC</td><td>152660339</td><td>Used as a clamping substrate when interfacing to mesh electronics I/O pads with the PCB-mounted ZIF connector</td></tr><tr><td>32-channel zero insertion force (ZIF) connector</td><td>Hirose Electric Co., LTD</td><td>FH12A-32S-0.5SH(55)</td><td>Component assembled onto the PCB</td></tr></tbody></table>

syringe-injectable mesh electronics for stable chronic rodent electrophysiology

Implantable brain electrophysiology probes are valuable tools in neuroscience due to their ability to record neural activity with high spatiotemporal resolution from shallow and deep brain regions. Their use has been hindered, however, by mechanical and structural mismatches between the probes and brain tissue that commonly lead to micromotion and gliosis with resulting signal instability in chronic recording experiments. In contrast, following the implantation of ultraflexible mesh electronics via syringe injection, the mesh probes form a seamless, gliosis-free interface with the surrounding brain tissue that enables stable tracking of individual neurons on at least a year timescale. This protocol details the key steps in a typical mouse neural recording experiment using syringe-injectable mesh electronics, including the fabrication of mesh electronics in a standard photolithography-based process possible at many universities, loading mesh electronics into standard capillary needles, stereotaxic injection in vivo, connection of the mesh input/output to standard instrumentation interfaces, restrained or freely moving recording sessions, and histological sectioning of brain tissue containing mesh electronics. Representative neural recordings and histology data are presented. Investigators familiar with this protocol will have the knowledge necessary to incorporate mesh electronics into their own experiments and take advantage of the unique opportunities afforded by long-term stable neural interfacing, such as studies of aging processes, brain development, and the pathogenesis of brain disease.

Results will vary based on the animal species in the study, the targeted brain region, the elapsed time since injection, the amount of acute damage inflicted during injection, and the success of the I/O interfacing procedure, among other factors. Single-unit spiking activity may not appear until 1 day (in the case of 150 &#181;m inner diameter needles) to 1 week after the injection and spike amplitudes can vary for up to 4&#8211;6 weeks. Figure 9 shows representative electrophysiological data from a 32-channel mesh electronics probe injected into the hippocampus and primary somatosensory cortex of an adult male C57BL/6J mouse. Approximately 300-&#181;V amplitude local field potentials (LFPs) were recorded on all 32 channels and single-unit spiking activity was recorded on 26 channels. The LFPs and isolated spikes remained similar between 2 and 4 months, suggesting a highly stable interface between recording electronics and neurons over this extended time period. Figure 10 shows representative results of histological sectioning and immunostaining of brain tissue containing mesh electronics 1 year after injection. Staining for NeuN, a marker for neural somata, and neurofilament, a marker for neural axons, reveals little to no loss of tissue density at the injection site, implying seamless interfacing between the mesh electronics and brain tissue. Staining for GFAP (a marker for astrocytes) further reveals near-background levels of astrocytes around mesh electronics, indicating that its presence elicits little chronic immune response.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/58003/58003fig1.jpg" /> 
Figure 1: Steps in a syringe-injectable mesh electronics experiment. This protocol describes all key steps in a typical rodent neural recording experiment using mesh electronics. Experiments usually entail, in order of implementation, (1) fabrication of mesh electronics, (2) loading of mesh electronics into capillary needles, (3) stereotaxic injection of mesh electronics into the brain, (4) electrical I/O interfacing to mesh electronics, (5) restrained or freely moving recordings, and (6) mesh/tissue sectioning and staining for histology. In some studies, only histology data may be desired, in which case steps (4) and (5) can be skipped. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig1large.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/58003/58003fig2.jpg" /> 
Figure 2: Schematic depicting the fabrication procedure for plug-and-play mesh electronics in the ultraflexible device region (top row), stem interconnects region (middle row), and I/O region (bottom row). (A) SU-8 negative photoresist (red) is patterned with PL mask-1 to define the bottom passivating layer of each plug-and-play mesh electronics probe. (B) Patterning with PL mask-2, thermal evaporation, and metal lift-off define Au interconnects and I/O pads (gold). (C) Patterning with PL mask-3, electron beam evaporation, and metal lift-off define Pt electrodes (blue). (D) SU-8 negative photoresist (red) is patterned with PL mask-4 to define the top passivating layer. Openings in the SU-8 are left at each Pt electrode and I/O pad. (E) A completed mesh electronics probe with dashed boxes indicating the locations enlarged in the top, middle, and bottom rows. Photomask design files are available by request from the authors or from the resource site, meshelectronics.org. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig2large.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/58003/58003fig3.jpg" /> 
Figure 3: Photographs and optical microscope images of plug-and-play mesh electronics. (A) Tiled optical microscope images of a syringe-injectable mesh electronics probe with plug-and-play I/O. The probe was imaged after the completion of the fabrication steps in Figure 2 but prior to the release from the Ni-coated substrate. Dashed boxes correspond from left to right to the sections of the ultraflexible device region, stem, and I/O region magnified in C, D, and E, respectively. Scale bar = 1 mm. (B) Photograph of a 3 inch Si wafer containing 20 completed mesh electronics probes. Scale bar = 20 mm. (C) Optical microscope image of 20 &#181;m diameter Pt recording electrodes in the ultraflexible device region. Scale bar = 100 &#181;m. (D) Optical microscope image of high-density Au interconnects in the stem region. Each Au interconnect is electrically isolated and connects a&#160;single Pt electrode to a single I/O pad. Scale bar = 100 &#181;m. (E) Optical microscope image of I/O pads. Each pad consists of a collapsible mesh region and a continuous thin-film region located on the stem. Non-conducting SU-8 ribbons connect the mesh portions of the pads together to help maintain alignment. Scale bar = 200 &#181;m. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig3large.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/58003/58003fig4.jpg" /> 
Figure 4: Assembly of apparatus for holding capillary needles during injection. (A) Photograph of the components of the apparatus. The components include (1) a glass capillary needle, (2) a pipette holder, (3) a circular screw fastener for the pipette holder, and (4) a cone washer for the pipette holder. Items (2) through (4) are included with purchase of a pipette holder. The arrow marks the outlet of the pipette holder which needs to be glued closed with epoxy. (B) Photograph of the pipette holder after assembly and insertion of a glass capillary needle. The added epoxy is visible at the top outlet of the pipette holder (marked by arrow) and capillary tubing connects the pipette holder to a syringe (not shown). (C) Photograph of the pipette holder and the capillary needle after the attachment to the stereotaxic frame with a right-angle end clamp. Scale bars are 1 cm. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig4large.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/58003/58003fig5.jpg" /> 
Figure 5: Loading of mesh electronics into glass needles. (A) Schematic illustration of the loading procedure for plug-and-play mesh electronics. A glass needle is positioned near the I/O end of a mesh electronics probe while it is suspended in solution. The syringe plunger is then manually retracted to draw in the mesh electronics probe. Ideal positioning is with the ultraflexible device region just inside the end of the needle. (B) Photographs corresponding to (A) of a mesh electronics probe being loaded into a glass needle. Scale bars = 2 mm. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig5large.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/58003/58003fig6.jpg" /> 
Figure 6: Schematic of the stereotaxic surgery station. A motorized stereotaxic frame (A) with attached pipette holder is used to position the needle into the desired brain region. The position of the needle and loaded mesh electronics are monitored with an objective lens and attached camera (B) and displayed on a computer (C). A syringe pump (D) flows precise volumes of saline through the needle, allowing for accurate, controlled injection of mesh electronics into the desired brain region. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig6large.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/58003/58003fig7.jpg" /> 
Figure 7: Plug-and-play I/O interfacing procedure. (A) An FFC clamping substrate is secured with dental cement adjacent to the craniotomy. (B) Plug-and-play mesh electronics are stereotaxically injected into the desired brain region using the FoV method. (C) The needle, with the I/O pads of the mesh electronics probe still inside, is repositioned over the FFC clamping substrate. (D) Flow is resumed through the needle to eject the I/O pads onto the FFC clamping substrate. (E) The I/O pads are bent 90&#176; relative to the stem, unfolded with the conducting side facing up, and dried in place. (F) The FFC substrate is trimmed with scissors to a straight-line ca. 0.5 mm from the edge of the I/O pads. Excess substrate is cut away to allow the insertion into a 32-channel ZIF connector. (G) The I/O pads are inserted into a 32-channel ZIF connector mounted on a custom PCB. The ZIF connector is latched closed to make contact with the I/O pads. (H) The latch is cemented closed, the PCB is flipped onto the skull, and the PCB is fixed in place with dental cement. (I) The PCB forms a compact headstage with a standard amplifier connector for easy interfacing during recording sessions. Scale bars = 1 cm. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig7large.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/58003/58003fig8.jpg" /> 
Figure 8: Restrained and freely moving recordings. (A) Photograph of a male C57BL/6J mouse in a restrainer during a recording session. A 32-channel preamplifier PCB has been inserted into the standard amplifier connector. (B) Photograph of the same mouse with 32-channel preamplifier PCB during a freely moving recording experiment. Scale bars = 1 cm. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig8large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 9" class="xfigimg" src="/files/ftp_upload/58003/58003fig9.jpg" /> 
Figure 9: Representative neural recording results. (A) Representative LFP heat maps from 32-channel mesh electronics probes injected into the mouse hippocampus and somatosensory cortex. Data were recorded while the mouse freely explored its cage at 2 months (top) and 4 months (bottom) post-injection. LFP amplitude is color-coded according to the color bar at right. High-pass filtered traces (black) showing spiking activity are overlaid on the spectrogram for each of the 32 channels. (B) Spikes isolated after sorting the data plotted in (A). Single-unit spiking activity was detected on 26 of the 32 channels both 2 months post-injection (top) and 4 months post-injection (bottom). The numbers above each cluster of spikes correspond to the channel numbers in (A). This figure has been modified from Fu, et al.28. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig9large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 10" class="xfigimg" src="/files/ftp_upload/58003/58003fig10.jpg" /> 
Figure 10: Representative histology results. (A) Schematic illustrating the orientation of mesh electronics within horizontal (middle panel) and sagittal (bottom panel) brain slices. (B) Fluorescence microscope image of a 10 &#181;m thick cortical brain slice one year after injection of a 16-channel mesh electronics probe. The slice has been immunostained for NeuN (green). (C) The same brain slice immunostained for neurofilament (red). (D) The same brain slice immunostained for GFAP (cyan). (E) A composite image of (B) through (D) showing the mesh electronics/tissue interface with labeled NeuN (green), neurofilament (red), GFAP (cyan), and mesh electronics (blue). Scale bars = 100 &#181;m. This figure has been modified from Fu et al.27. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/58003fig10large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
Supplementary Video 1: Repeated loading and injection of mesh electronics into solution. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58003/video1.mp4">Please click here to download this file.</a>

Watch this Scientific Journal Video about Syringe-injectable Mesh Electronics for Stable Chronic Rodent Electrophysiology at JoVE.com

Syringe-injectable Mesh Electronics for Stable Chronic Rodent Electrophysiology

Mesh electronics probes seamlessly integrate and provide stable, long-term, single-neuron level recording within the brain. This protocol uses mesh electronics for in vivo experiments, involving the fabrication of mesh electronics, loading into needles, stereotaxic injection, input/output interfacing, recording experiments, and histology of tissue containing mesh probes.

Implantable brain electrophysiology probes are valuable tools in neuroscience due to their ability to record neural activity with high spatiotemporal ...

syringe-injectable-mesh-electronics-for-stable-chronic-rodent

Universidad de Cartagena UDEC

Research

JoVE Journal

Bioengineering

23.0K Views.  Harvard University. Mesh electronics probes seamlessly integrate and provide stable, long-term, single-neuron level recording within the brain. This protocol uses mesh electronics for in vivo experiments, involving the fabrication of mesh electronics, loading into needles, stereotaxic injection, input/output interfacing, recording experiments, and histology of tissue containing mesh probes.

Video: Syringe-injectable Mesh Electronics for Stable Chronic Rodent Electrophysiology

In vivo Optogenetic Stimulation of the Rodent Central Nervous System

The ability to probe defined neural circuits in awake, freely-moving animals with cell-type specificity, spatial precision, and high temporal resolution has been a long sought tool for neuroscientists in the systems-level search for the neural circuitry governing complex behavioral states. Optogenetics is a cutting-edge tool that is revolutionizing the field of neuroscience and represents one of the first systematic approaches to enable causal testing regarding the relation between neural signaling events and behavior. By combining optical and genetic approaches, neural signaling can be bi-directionally controlled through expression of light-sensitive ion channels (opsins) in mammalian cells. The current protocol describes delivery of specific wavelengths of light to opsin-expressing cells in deep brain structures of awake, freely-moving rodents for neural circuit modulation. Theoretical principles of light transmission as an experimental consideration are discussed in the context of performing in vivo optogenetic stimulation. The protocol details the design and construction of both simple and complex laser configurations and describes tethering strategies to permit simultaneous stimulation of multiple animals for high-throughput behavioral testing.

In vivo Optogenetic Stimulation of the Rodent Central Nervous System

Optogenetics has become a powerful tool for use in behavioral neuroscience experiments. This protocol offers a step-by-step guide to the design and set-up of laser systems, and provides a full protocol for carrying out multiple and simultaneous in vivo optogenetic stimulations compatible with most rodent behavioral testing paradigms.

The ability to probe defined neural circuits in awake, freely-moving animals with cell-type specificity, spatial precision, and high temporal resolution ...

Neuroscience

Simultaneous Electrophysiological Recording and Micro-injections of Inhibitory Agents in the Rodent Brain

Here we describe a method for the construction of a single-use &#8220;injectrode&#8221; using commercially accessible and affordable parts. A probing system was developed that allows for the injection of a drug while recording electrophysiological signals from the affected neuronal population. This method provides a simple and economical alternative to commercial solutions. A glass pipette was modified by combining it with a hypodermic needle and a silver filament. The injectrode is attached to commercial microsyringe pump for drug delivery. This results in a technique that provides real-time pharmacodynamics feedback through multi-unit extracellular signals originating from the site of drug delivery. As a proof of concept, we recorded neuronal activity from the superior colliculus elicited by flashes of light in rats, concomitantly with delivery of drugs through the injectrode. The injectrode recording capacity permits the functional characterization of the injection site favoring precise control over the localization of drug delivery. Application of this method also extends far beyond what is demonstrated here, as the choice of chemical substance loaded into the injectrode is vast, including tracing markers for anatomic experiments.

Here, we craft a glass pipette with dual functions: inhibition of deep brain structures by microinjections of drugs and real-time monitoring of their effects through simultaneous electrophysiological recordings.

Here we describe a method for the construction of a single-use &#8220;injectrode&#8221; using commercially accessible and affordable parts. A probing ...

Long-term Continuous EEG Monitoring in Small Rodent Models of Human Disease Using the Epoch Wireless Transmitter System

Many progressive neurologic diseases in humans, such as epilepsy, require pre-clinical animal models that slowly develop the disease in order to test interventions at various stages of the disease process. These animal models are particularly difficult to implement in immature rodents, a classic model organism for laboratory study of these disorders. Recording continuous EEG in young animal models of seizures and other neurological disorders presents a technical challenge due to the small physical size of young rodents and their dependence on the dam prior to weaning. Therefore, there is not only a clear need for improving pre-clinical research that will better identify those therapies suitable for translation to the clinic but also a need for new devices capable of recording continuous EEG in immature rodents. Here, we describe the technology behind and demonstrate the use of a novel miniature telemetry system, specifically engineered for use in immature rats or mice, which is also effective for use in adult animals.

Here we demonstrate the use of a wireless enabling technology for electroencephalogram (EEG) in neonatal rodent models of human disease. With telemetry, there are no encumbering connections, thus allowing natural behaviors.

Many progressive neurologic diseases in humans, such as epilepsy, require pre-clinical animal models that slowly develop the disease in order to test ...

Novel Approach for Simultaneous Recording of Renal Sympathetic Nerve Activity and Blood Pressure with Intravenous Infusion in Conscious, Unrestrained Mice.

Renal sympathetic nerves contribute significantly to both physiological and pathophysiological phenomena. Evaluating renal sympathetic nerve activity (RSNA) is of great interest in many areas of research such as chronic kidney disease, hypertension, heart failure, diabetes and obesity. Unequivocal assessment of the role of the sympathetic nervous system is thus imperative for proper interpretation of experimental results and understanding of disease processes. RSNA has been traditionally measured in anesthetized rodents, including mice. However, mice usually exhibit very low systemic blood pressure and hemodynamic instability for several hours during anesthesia and surgery. Meaningful interpretation of RSNA is confounded by this non-physiological state, given the intimate relationship between sympathetic nervous tone and cardiovascular status. To address this limitation of traditional approaches, we developed a new method for measuring RSNA in conscious, freely-moving mice. Mice were chronically instrumented with radio-telemeters for continuous monitoring of blood pressure as well as a jugular venous infusion catheter and custom-designed bipolar electrode for direct recording of RSNA. Following a 48-72 hour recovery period, survival rate was 100% and all mice behaved normally. At this time-point, RSNA was successfully recorded in 80% of mice, with viable signals acquired up to 4 and 5 days post-surgery in 70% and 50% of mice, respectively. Physiological blood pressures were recorded in all mice (116&plusmn;2 mmHg; n=10). Recorded RSNA increased with eating and grooming, as well-established in the literature. Furthermore, RSNA was validated by ganglionic blockade and modulation of blood pressure with pharmacological agents. Herein, an effective and manageable method for clear recording of RSNA in conscious, freely-moving mice is described.

Anesthetized mice exhibit non-physiological systemic blood pressure, which precludes meaningful assessment of autonomic tone given the intimate relationship between blood pressure and the autonomic nervous system. Thus, a novel method to simultaneously record renal sympathetic nerve activity and blood pressure with intravenous infusion in conscious mice is outlined.

Renal sympathetic nerves contribute significantly to both physiological and pathophysiological phenomena. Evaluating renal sympathetic nerve activity ...

Medicine

Chronic Implantation of Multiple Flexible Polymer Electrode Arrays

Simultaneous recordings from large populations of individual neurons across distributed brain regions over months to years will enable new avenues of scientific and clinical development. The use of flexible polymer electrode arrays can support long-lasting recording, but the same mechanical properties that allow for longevity of recording make multiple insertions and integration into a chronic implant a challenge. Here is a methodology by which multiple polymer electrode arrays can be targeted to a relatively spatially unconstrained set of brain areas.
The method utilizes thin-film polymer devices, selected for their biocompatibility and capability to achieve long-term and stable&#160;electrophysiologic recording interfaces. The resultant implant allows accurate and flexible targeting of anatomically distant regions, physical stability for months, and robustness to electrical noise. The methodology supports up to sixteen serially inserted devices across eight different anatomic targets. As previously demonstrated, the methodology is capable of recording from 1024 channels. Of these, the 512 channels in this demonstration used for single neuron recording yielded 375 single units distributed across six recording sites. Importantly, this method also can record single units for at least 160 days.
This implantation strategy, including temporarily bracing each device with a retractable silicon insertion shuttle, involves tethering of devices at their target depths to a skull-adhered plastic base piece that is custom-designed for each set of recording targets, and stabilization/protection of the devices within a silicone-filled, custom-designed plastic case. Also covered is the preparation of devices for implantation, and design principles that should guide adaptation to different combinations of brain areas or array designs.

Described below is a method for implantation of multiple polymer electrode arrays across anatomically distant brain regions for chronic electrophysiological recording in freely moving rats. Preparation and surgical implantation are described in detail, with emphasis on design principles to guide adaptation of these methods for use in other species.

Simultaneous recordings from large populations of individual neurons across distributed brain regions over months to years will enable new avenues of ...

An Implantable System For Chronic In Vivo Electromyography

Electromyography (EMG) measures the muscle response to electrical stimulation or spontaneous activity of motor units and plays an important role in assessing neuromuscular function. Chronic recording of EMG activity reflecting a muscle&#8217;s reinnervation status after nerve injury has been limited, due to the invasive nature of traditional EMG recording techniques. In this regard, an implantable system is designed for long-term, in vivo EMG recording and nerve stimulation. It has been applied and tested in a study on reinnervation of laryngeal muscles. This system consists of 1) two bipolar electrode nerve cuffs and leads for stimulating each of two nerves: the recurrent laryngeal nerve (RLN) and internal branch of the superior laryngeal nerve (SLN); 2) two EMG recording electrodes and leads for each of the two laryngeal muscles: posterior cricoarytenoid (PCA) muscle and thyroarytenoid-lateral cricoarytenoid (TA-LCA) muscle complex; and 3) a skin receptacle interfacing all implanted lead terminals to an external recording preamplifier and stimulator using a connection cable. The wire leads are Teflon-coated, multi-filament, type 316 stainless steel. They are coiled and can stretch during body movement of the awake animal to prevent lead breakage and electrode migration. This system is implanted during an aseptic surgery. Afterwards, baseline EMG recordings are performed before the RLN is transected in the second surgery to study muscle reinnervation. Throughout the study, multiple physiological sessions are conducted in the anesthetized animal to obtain evoked and spontaneous EMG activity that reflects the reinnervation status of laryngeal muscles. The system is compact, free of infection over the course of the study, and highly durable. This implantable system can provide a reliable platform for research in which long-term recording or nerve stimulation is required in an anesthetized or freely moving animal.&#160;

Presented here is a protocol for the manufacturing of an implantable system for in vivo chronological recording of evoked and spontaneous electromyographic potentials. The system is applied to the investigation of reinnervation of laryngeal muscles following nerve injury. &#160;&#160;

Electromyography (EMG) measures the muscle response to electrical stimulation or spontaneous activity of motor units and plays an important role in ...

Microinjectrode System for Combined Drug Infusion and Electrophysiology

This microinjectrode system is designed for drug infusion, electrophysiology, and delivery and retrieval of experimental probes, such as microelectrodes and nanosensors, optimized for repeated use in awake, behaving animals. The microinjectrode system can be configured for multiple purposes: (1) simple arrangement of the cannula for placement of an experimental probe that would otherwise be too fragile to penetrate the dura mater, (2) microfluidic infusion of a drug, either independently or coupled to a cannula containing an experimental probe (i.e., microelectrode, nanosensor). In this protocol we explain the step by step construction of the microinjectrode, its coupling to microfluidic components, and the protocol for use of the system in vivo. The microfluidic components of this system allow for delivery of volumes on the nanoliter scale, with minimal penetration damage. Drug infusion can be performed independently or simultaneously with experimental probes such as microelectrodes or nanosensors in an awake, behaving animal. Applications of this system range from measuring the effects of a drug on cortical electrical activity and behavior, to understanding the function of a specific region of cortex in the context of behavioral performance based on probe or nanosensor measurements. To demonstrate some of the capabilities of this system, we present an example of muscimol infusion for reversible inactivation of the frontal eye field (FEF) in rhesus macaque during a working memory task.

We present a microinjectrode system designed for electrophysiology and assisted delivery of experimental probes (i.e., nanosensors, microelectrodes), with optional drug infusion. Widely available microfluidic components are coupled to a cannula containing the probe. A step-by-step protocol for microinjectrode construction is included, with results during muscimol infusion in macaque cortex.

This microinjectrode system is designed for drug infusion, electrophysiology, and delivery and retrieval of experimental probes, such as microelectrodes ...

Open&#45;Source Implant for Multi&#45;Region Electrophysiological Monitoring in Rats

The TD Drive: A Parametric, Open-Source Implant for Multi&#45;Area Electrophysiological Recordings in Behaving and Sleeping Rats

Intricate interactions between multiple brain areas underlie most functions attributed to the brain. The process of learning, as well as the formation and consolidation of memories, are two examples that rely heavily on functional connectivity across the brain. In addition, investigating hemispheric similarities and/or differences goes hand in hand with these multi-area interactions. Electrophysiological studies trying to further elucidate these complex processes thus depend on recording brain activity at multiple locations simultaneously and often in a bilateral fashion. Presented here is a 3D-printable implant for rats, named TD Drive, capable of symmetric, bilateral wire electrode recordings, currently in up to ten distributed brain areas simultaneously. The open-source design was created employing parametric design principles, allowing prospective users to easily adapt the drive design to their needs by simply adjusting high-level parameters, such as anterior-posterior and mediolateral coordinates of the recording electrode locations. The implant design was validated in n = 20 Lister Hooded rats that performed different tasks. The implant was compatible with tethered sleep recordings and open field recordings (Object Exploration) as well as wireless recording in a large maze using two different commercial recording systems and headstages. Thus, presented here is the adaptable design and assembly of a new electrophysiological implant, facilitating fast preparation and implantation.

Author Spotlight: Deciphering Memory and Learning Through Neural Implants for Multi&#45;Region Brain Studies

Here, we present a unique, 3D-printable implant for rats, named TD Drive, capable of symmetric, bilateral wire electrode recordings, currently in up to ten distributed brain areas simultaneously.

Intricate interactions between multiple brain areas underlie most functions attributed to the brain. The process of learning, as well as the formation and ...

A Cost-Effective, Versatile Probe Implant System for Electrophysiology in Mice

The DREAM Implant: A Lightweight, Modular, and Cost-Effective Implant System for Chronic Electrophysiology in Head-Fixed and Freely Behaving Mice

Chronic electrophysiological recordings in rodents have significantly improved our understanding of neuronal dynamics and their behavioral relevance. However, current methods for chronically implanting probes present steep trade-offs between cost, ease of use, size, adaptability, and long-term stability.
This protocol introduces a novel chronic probe implant system for mice called the DREAM (Dynamic, Recoverable, Economical, Adaptable, and Modular), designed to overcome the trade-offs associated with currently available options. The system provides a lightweight, modular and cost-effective solution with standardized hardware elements that can be combined and implanted in straightforward steps and explanted safely for recovery and multiple reuse of probes, significantly reducing experimental costs.
The DREAM implant system integrates three hardware modules: (1) a microdrive that can carry all standard silicon probes, allowing experimenters to adjust recording depth across a travel distance of up to 7 mm; (2) a three-dimensional (3D)-printable, open-source design for a wearable Faraday cage covered in copper mesh for electrical shielding, impact protection, and connector placement, and (3) a miniaturized head-fixation system for improved animal welfare and ease of use. The corresponding surgery protocol was optimized for speed (total duration: 2 h), probe safety, and animal welfare.
The implants had minimal impact on animals&#39; behavioral repertoire, were easily applicable in freely moving and head-fixed contexts, and delivered clearly identifiable spike waveforms and healthy neuronal responses for weeks of post-implant data collection. Infections and other surgery complications were extremely rare.
As such, the DREAM implant system is a versatile, cost-effective solution for chronic electrophysiology in mice, enhancing animal well-being, and enabling more ethologically sound experiments. Its design simplifies experimental procedures across various research needs, increasing accessibility of chronic electrophysiology in rodents to a wide range of research labs.

Here, we introduce a lightweight, cost-effective probe implant system for chronic electrophysiology in rodents optimized for ease of use, probe recovery, experimental versatility, and compatibility with behavior.

Chronic electrophysiological recordings in rodents have significantly improved our understanding of neuronal dynamics and their behavioral relevance. ...

Injectable Mesh Electronics for Stable Single-Neuron Recordings in a Mouse Brain

Source: Schuhmann Jr., T. G., et al. <a href="https://appjove.unicartagenaproxy.elogim.com/v/58003">Syringe-injectable Mesh Electronics for Stable Chronic Rodent Electrophysiology.</a> J. Vis. Exp. (2018).
The video demonstrates the injection of mesh electronics probes into a mouse brain for stable long-term recordings at a single-neuron level. An anesthetized mouse with an exposed skull is secured on a stereotaxic frame, and the probe&#39;s mesh device region is injected into the brain through drilled holes. The probe&#39;s input-output pads are connected to a circuit, and recordings are obtained using a data acquisition system.

1. Stereotaxic Injection of Mesh Electronics into Live Mouse Brain
NOTE: Mice were anesthetized by intraperitoneal injection with a mixture of 75 mg/kg ...

Syringe-injectable Mesh Electronics for Stable Chronic Rodent Electrophysiology

Summary

Explore More Videos

Chapters in this video

In vivo Optogenetic Stimulation of the Rodent Central Nervous System

Simultaneous Electrophysiological Recording and Micro-injections of Inhibitory Agents in the Rodent Brain

Long-term Continuous EEG Monitoring in Small Rodent Models of Human Disease Using the Epoch Wireless Transmitter System

Novel Approach for Simultaneous Recording of Renal Sympathetic Nerve Activity and Blood Pressure with Intravenous Infusion in Conscious, Unrestrained Mice.

Chronic Implantation of Multiple Flexible Polymer Electrode Arrays

An Implantable System For Chronic In Vivo Electromyography

Microinjectrode System for Combined Drug Infusion and Electrophysiology

The TD Drive: A Parametric, Open-Source Implant for Multi-Area Electrophysiological Recordings in Behaving and Sleeping Rats

The DREAM Implant: A Lightweight, Modular, and Cost-Effective Implant System for Chronic Electrophysiology in Head-Fixed and Freely Behaving Mice

Injectable Mesh Electronics for Stable Single-Neuron Recordings in a Mouse Brain