Name: focused ultrasound neuromodulation of human in vitro neural cultures in multi-well microelectrode arrays
Uploaded: 2024-05-03T12:40:00
Duration: 4 min
Description: Watch this Scientific Journal Video about Focused Ultrasound Neuromodulation of Human In Vitro Neural Cultures in Multi-Well Microelectrode Arrays at JoVE.com

Amir Manbachi and Nitish Thakor acknowledge funding support from the Defense Advanced Research Projects Agency, DARPA, Award Contract: N660012024075. In addition, Amir Manbachi acknowledges funding support from the Johns Hopkins Institute for Clinical and Translational Research (ICTR)&#39;s Clinical Research Scholars Program (KL2), administered by the National Center for Advancing Translational Sciences (NCATS), National Institutes of Health (NIH). Nitish Thakor acknowledges funding support from the National Institutes of Health (NIH): R01 HL139158-01A1 and R01 HL071568-15.

1. Preparation of materials
<ol>
	<li>Aspirate the culture medium, and use it to fill a single well in a 24-well neuron culture plate with embedded MEA (Figure 2A). Culture and induce the neurons following the published protocol by Taga et al.13.</li>
	<li>Sterilize the parafilm interface, the rubber band, and the FUS cone with its rubber membrane using 70% ethanol for 10 min, and place them in the fume hood for later assembly.</li>
	<li>Degas 300 mL of deionized water and 50 mL of coupling gel. Centrifuge the water and gel at 160 x g for 5 min to avoid inducing cavitation within the coupling medium. 
	NOTE: The original source of the HiPSCs is from GM01582 and CIPS cell lines. On average, a density of 5 x 104 motor neurons and 2.5 x 104 astrocytes per well can be achieved14.</li>
</ol>
2. Connection and setup of the peripherals
<ol>
	<li>Secure the FUS cone to the transducer using screws, and seal the cone with a flexible rubber membrane in a ventilated sterile hood. Fill the cone with the degassed and deionized (DG-DI) water from step 1.3, and ensure the absence of bubbles in the cone to avoid cavitation.</li>
	<li>Use a customized threaded rod to secure the 3D-printed holder to a frame (Figure 2B). Position the frame such that the head of the FUS transducer is over the well that will be stimulated.</li>
	<li>Use a rubber band to secure parafilm over the well on the 24-well MEA plate containing the medium and the HiPSCs.</li>
	<li>Prepare the FUS system by connecting the ultrasound transducer&#39;s back-end driver electronics, in this case, the transducer power output (TPO; Figure 3A), to a 100-240 V power outlet (Figure 3B, Connection 6) and connecting the matching network to the TPO and the FUS transducer (Figure 3B, Connection 1 and Connection 2, respectively). The matching network ensures efficient electrical coupling between the transducer and the TPO.</li>
	<li>Connect the MEA system to a power outlet (100-240 V) (Figure 3B, Connection 5). Connect the MEA system synchronization port to the TPO (Figure 3B, Connection 3). This connection will synchronize the data acquisition by the MEA system with the FUS stimulation.</li>
	<li>Place the 24-well MEA plate in the MEA system, and remove the lid to enable direct contact between the transducer and the well. Place the transducer 5-10 mm above the well plate to allow room for the degassed coupling gel, as described in step 3.2 (Figure 3A and Figure 2B).</li>
</ol>
3. Stimulation and neuronal signal acquisition
<ol>
	<li>Set the FUS parameters on the TPO control panel&#160; (Table&#160;1).</li>
	<li>Apply the coupling gel on top of the parafilm, and lower the FUS transducer into the coupling gel, ensuring contact with the gel with minimal air bubbles (Figure 2A).</li>
	<li>Start the MEA system recording by clicking on the Start button on the user interface.</li>
	<li>Start the FUS sonication by pressing the bottom right button on the TPO (Figure 3A, Label 7), and wait at least 5 min between each round of sonication to allow the neurons to return to a baseline state.</li>
	<li>Use the trigger pulse generated by the FUS system to align the FUS stimulation sequence to the MEA recording (Figure 3B, Connection 3).</li>
</ol>
4. Data processing and analysis
<ol>
	<li>Transfer the data from the MEA system to the computer using a USB connection (Figure 3B, Connection 4). Start this by clicking on the Experiment Set Up panel. Next, choose the data type one wishes to record. In this case, raw spikes are recommended. Finally, name the file, and select the desired location within the disk drive to complete the transfer. 
	NOTE: The following steps can be performed by running the released Python script in&#160;https://github.com/Rxliang/FUSNeuromod.</li>
	<li>Read in the data from each of the 16 electrodes.</li>
	<li>Apply a Butterworth bandpass filter with a 5 Hz to 3 kHz bandwidth with a Butterworth order of 8. 
	NOTE: To optimize these values, it is crucial to take into account the firing rate of the specific cells and the number of cells involved. By multiplying these&#160;2 values, one can estimate the overall firing rate of the cell population in the experiment.</li>
	<li>Apply a Gaussian filter with &#963; = 3 to smooth the signal. 
	NOTE: The parameter could be optimized based on the recommended values from the MEA system, as excessive smoothing may result in data distortion after acquisition, and too little smoothing would introduce unwanted noise.</li>
	<li>Set a threshold to detect the potential spikes as 5 times the standard deviation of the Gaussian-smoothed signal.</li>
	<li>Compute the firing rate by dividing the number of spikes registered in a 50 ms window across all 16 channels by the length of the window (i.e., 50 ms). Shift the window along the signal to the next frame, and repeat the firing rate calculation (Supplementary Figure 1).</li>
	<li>Analyze the signal by reading the FUS sonication time from the transferred data based on the change in the firing rate associated with the FUS.</li>
</ol>
5. Multi-well MEA plate cleaning and reuse
<ol>
	<li>Once the experiments are complete, use a pipette to carefully remove the medium from the wells in the multi-well plate, taking care to avoid the electrode surface.</li>
	<li>Add 2 mL of DG-DI water per well. Aspirate and repeat once.</li>
	<li>To dislodge any cells and debris, add a mixture of 1 g of enzymatic detergent Terg-A-Zyme with 10 mL of sterile DG-DI water (0.3 mL per well) to the plate. Leave it to incubate overnight at room temperature (RT).</li>
	<li>The following day, remove the solution from the wells, and rinse them with 1 mL of sterile DG-DI water.</li>
	<li>Incubate the multi-well plate for 5-7 min, and aspirate. Repeat this step 5 times.</li>
	<li>Add 0.5 mL of sterile DG-DI water per well. Record the baseline of the cleaned multi-well plate to validate that the MEA plate is clean. A cleaned plate should exhibit Gaussian noise patterns with low intensity values.</li>
	<li>Store the cleaned multi-well plate at 4 &#176;C until it is ready to be used again. Change the water the MEAs are stored in at least once per month.</li>
</ol>

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Opt. 15 (2), 021314 (2010).</li><li>Akhtar, K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Noninvasive+peripheral+focused+ultrasound+neuromodulation+of+the+celiac+plexus+ameliorates+symptoms+in+a+rat+model+of+inflammatory+bowel+disease.">Noninvasive peripheral focused ultrasound neuromodulation of the celiac plexus ameliorates symptoms in a rat model of inflammatory bowel disease.</a> Experimental Physiology. 106 (4), 1038-1060 (2021).</li><li>Smirnova, L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Organoid+intelligence+(OI):+The+new+frontier+in+biocomputing+and+intelligence-in-a-dish.">Organoid intelligence (OI): The new frontier in biocomputing and intelligence-in-a-dish.</a> Frontiers in Science. 1, 1017235 (2023).</li><li>Saccher, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Focused+ultrasound+neuromodulation+on+a+multi-well+MEA.">Focused ultrasound neuromodulation on a multi-well MEA.</a> Bioelectronic Medicine. 8 (1), 2 (2022).</li><li>Yger, P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+spike+sorting+toolbox+for+up+to+thousands+of+electrodes+validated+with+ground+truth+recordings+in+vitro+and+in+vivo.">A spike sorting toolbox for up to thousands of electrodes validated with ground truth recordings in vitro and in vivo.</a> eLife. 7, e34518 (2018).</li><li>Babakhanian, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Effects+of+low+intensity+focused+ultrasound+on+liposomes+containing+channel+proteins.">Effects of low intensity focused ultrasound on liposomes containing channel proteins.</a> Scientific Reports. 8, 17250 (2018).</li><li>Liang, R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Designing+an+Accurate+Benchtop+Characterization+Device:+An+acoustic+measurement+platform+for+localizing+and+implementing+therapeutic+ultrasound+devices+and+equipment+(amplitude).">Designing an Accurate Benchtop Characterization Device: An acoustic measurement platform for localizing and implementing therapeutic ultrasound devices and equipment (amplitude).</a> 2022 Design of Medical Devices Conference. , (2022).</li><li>Ko, H., Yoon, S. -. 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The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest. Amir Manbachi teaches and consults for BK Medical (GE Healthcare) and Neurosonics Medical and is an inventor on a number of patent-pending FUS technologies. Betty Tyler has research funding from NIH and is a co-owner of Accelerating Combination Therapies (including equity or options). Ashvattha Therapeutics Inc. has licensed one of her patents and&#160;she is a stockholder for Peabody Pharmaceuticals.

This manuscript describes a novel method that can be used to record neuronal activity in HiPSCs during FUS neuromodulation. This protocol is generalizable to different FUS transducers and MEA systems. To replicate the results observed with the described protocol, the researcher should ensure that the focal point of the transducer is greater than the area of the bottom of the MEA well. Furthermore, if different neuronal cell lines are used, the filter parameters must be tuned to the expected frequency response for the cells within the well. If representative results cannot be achieved, one should consider modifying the aforementioned parameters (e.g., the burst length, intensity, duty cycle, etc.).
Though this work demonstrated an increase in the firing rate following FUS stimulation, more data must be collected to demonstrate the repeatability of this finding before any conclusions are drawn. This protocol inherits the limitations of MEA systems, which typically have weaknesses stemming from the direct microelectrode current signal recording. Though direct contact with the neuron provides better sensitivity, it may alter the cell and affect the measurement accuracy. Furthermore, due to the small size of the wells, our system does not include peripheral tissue, which may also play a role in neuromodulation17. This may limit the applicability of conclusions drawn from this setup to in vivo environments. To study more complex network responses, a higher-channel density MEA system must be designed to improve its sensitivity18. Several future directions for this proposed system have been identified, including using a 3D gantry to hold the transducer and ensure accurate placement19. Additional improvements could be made regarding the post-processing algorithm, including utilizing a spiking sorting algorithm20 to classify individual neurons. This process would be beneficial for disentangling the responses of multi-unit neurons in future studies on the mechanisms of FUS. Most importantly, it is essential to incorporate additional modalities of stimulation, such as chemical, electrical, and optical stimuli, to elucidate the underlying mechanisms. These methods can alter neuronal properties and behaviors, such as by inhibiting specific ion channels15 or modifying the membrane characteristics21. By modulating the main factors within the hypothesized signaling pathway, researchers can identify the contributions of each factor in controlled environments and, ultimately, shed light on the complex interactions at play.
Electrical stimulation22 is one of the most established techniques for neuromodulation, with a long history of successful applications in clinical and research settings. In contrast, FUS and optogenetics23 are relatively new modalities that have gained attention in recent years. The major advantages of FUS are its non-invasiveness and ability to stimulate neurons at depths that may be difficult to reach with other techniques, including electrical stimulation and optogenetics. However, like optogenetics24, FUS has some limitations related to modeling the wave propagation and associated neuronal responses. Capturing the complexity of tissue&#39;s heterogeneous acoustic properties in vivo can be challenging, which leads to uncertainties in the pressure field and, consequently, in the neuronal responses. This difficulty in accurately modeling these properties presents a challenge when optimizing the technique for specific real-world applications. The inherent complexities emphasize the importance of in vitro systems like the one in this study, as they enable the direct study of responses under controlled acoustic intensity conditions.
In conclusion, this system provides a high-throughput, in vitro platform for studying the neuro-modulatory effects of FUS on human neurons. With this system, the mechanisms of action of FUS can be explored by measuring the electrical responses from human neurons when exposed to varying levels and types of stimulation in a controlled environment. Therefore, it offers a valuable supplementary tool to the human and animal models commonly used in the field.

Focused ultrasound (FUS) is a promising neuromodulation modality that enables noninvasive stimulation at centimeter-level depths with sub-millimeter resolution1,2,3. Despite these strengths, the clinical impact of FUS is limited, in part due to a lack of knowledge regarding its mechanism of action. Without a solid theoretical foundation, researchers and clinicians face difficulties in tailoring the therapy to meet the specific needs of individual patients under varying conditions. A prominent theory proposed by Yoo et al.4 suggests that mechanosensitive ion channels are responsible for neuron activation. However, this theory fails to explain FUS activation in human brain neurons, which lack these channels5. This ambiguity limits the utilization of FUS in the clinic, as it precludes the tuning of FUS parameters to optimize treatment outcomes.
Prior related studies have employed a range of approaches to investigate the physiological mechanisms underpinning FUS&#160;and to determine the optimal stimulation parameters. A crucial step in this process involves monitoring neuronal responses as feedback, which can be achieved through methods involving ion-gate monitoring, such as calcium ion imaging4, optical imaging1, and ex vivo electrophysiological recording (e.g., electromyography6 or skin-nerve electrophysiology7). However, most of these studies use non-human neurons or in vivo approaches, which can introduce additional variances due to sub-optimal controls. In contrast, using electrodes to measure neuronal signals in in vitro&#160;human-induced pluripotent stem cell (HiPSC) neurons offers more sensitive measurements and greater control over the experimental environment. In this work, an in vitro system has been developed using micro-electrode arrays (MEAs) to measure the electrical responses of HiPSC neurons following FUS stimulation, as shown in Figure 1. This system empowers researchers in the community to monitor neuronal responses when varying the ultrasound parameters (e.g., frequency, burst length, intensity). Additionally, this system enables a high level of control of the neuronal sensitivity to physical stimuli (e.g., temperature, pressure, and cavitation)8,9, as the neurons&#39; ion channel functionality can be manipulated genetically and pharmaceutically (e.g., using gadolinium to inhibit ion channels)10,11,12. This molecular-level control may help to elucidate the mechanisms behind the neuromodulatory effects of FUS.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>MEA System</td>
			<td>Axion Biosystem Inc.</td>
			<td>Maestro Edge</td>
			<td>Sampling Rate: 11500 Hz</td>
		</tr>
		<tr>
			<td>MEA Plate</td>
			<td>Axion Biosystem Inc.</td>
			<td>CytoView MEA</td>
			<td>Electrode and Well: 16 electrodes in 24 wells</td>
		</tr>
		<tr>
			<td>Well plate Interface</td>
			<td>Amcor Inc.</td>
			<td>Parafilm PM996; P7793</td>
			<td>Thickness: 127 &#181;m</td>
		</tr>
		<tr>
			<td>CO2 Tank and Regulator for culture</td>
			<td>AirGas Inc./ Harris Inc.</td>
			<td>9296NC</td>
			<td>Concentration: 5%</td>
		</tr>
		<tr>
			<td>Culture Media</td>
			<td>ThermoFisher Inc.</td>
			<td>Laminin; 23017-015</td>
			<td>Concentration: 1 &#181;g/mL</td>
		</tr>
		<tr>
			<td>HiPSC Neurons</td>
			<td>Peprotech</td>
			<td>CIPS and GM01582 Derived; 450-10</td>
			<td>Concentration: 10 ng/mL (Refer Taga et al [2021]13)</td>
		</tr>
		<tr>
			<td>Transducer</td>
			<td>Sonic Concepts Inc.</td>
			<td>CTX250; 008</td>
			<td>Center Frequency: 250 kHz</td>
		</tr>
		<tr>
			<td>Matching Network</td>
			<td>Sonic Concepts Inc.</td>
			<td>CTX250; NFS102v2</td>
			<td>Impedance: 50 &#937;</td>
		</tr>
		<tr>
			<td>Transducer Power Output (TPO)</td>
			<td>Sonic Concepts Inc.</td>
			<td>Version 4.1; 020</td>
			<td>Frequency: From 250 kHz to 2.5 MHz</td>
		</tr>
		<tr>
			<td>Membrane</td>
			<td>McMaster Inc.</td>
			<td>Silicone Rubber; 5542N115</td>
			<td>Thickness: 0.0127 cm</td>
		</tr>
		<tr>
			<td>Coupling Gel</td>
			<td>Parker Laboratory Inc.</td>
			<td>Aquasonic 100; B08DDWG GXB</td>
			<td>Viscosity: 130,000&#8211;185,000 cops</td>
		</tr>
		<tr>
			<td>Connection to Probe holder</td>
			<td>McMaster Inc.</td>
			<td>Steal Threaded Rod; 90322A661</td>
			<td>Length: 1&#8211;1/2&#34; Long</td>
		</tr>
		<tr>
			<td>Centrifuge</td>
			<td>ThermoFisher Inc.</td>
			<td>Sorvall Legend X1R; 75004261</td>
			<td>Max acceleration: 10&#8211;25,830 x g</td>
		</tr>
		<tr>
			<td>Hydrophone</td>
			<td>Sonic Concepts Inc.</td>
			<td>Y-104; 009</td>
			<td>Range: 50 kHz&#8211;1.9 MHz</td>
		</tr>
		<tr>
			<td>Water Tank</td>
			<td>Sonic Concepts Inc.</td>
			<td>WT</td>
			<td>Size: 30 cm x 30 cm x 30 cm</td>
		</tr>
		<tr>
			<td>Water Conditioning Unit</td>
			<td>Sonic Concepts Inc.</td>
			<td>WCU; SN006</td>
			<td>Flow Velocity: 50 mL/s maximum</td>
		</tr>
		<tr>
			<td>Oscilloscope</td>
			<td>Rohde-Schwarz Inc.</td>
			<td>RTC1002</td>
			<td>Sampling rate: Up to 50 MHz</td>
		</tr>
		<tr>
			<td>Stage</td>
			<td>Sonic Concepts Inc.</td>
			<td>MicroStage; 2</td>
			<td>Accuracy: 1 &#181;m</td>
		</tr>
		<tr>
			<td>Thermochromic sheet</td>
			<td>TIPTEMP Inc.</td>
			<td>Liquid Crystal Sheet; TLCSEN337</td>
			<td>Range: 22&#8211;24 &#176;C</td>
		</tr>
		<tr>
			<td>Computer</td>
			<td>Microsoft Surface</td>
			<td>Surface Pro</td>
			<td>CPU i5 1035G4: 3.7 GHz</td>
		</tr>
		<tr>
			<td>Data Transfer Software</td>
			<td>Mathworks Inc.</td>
			<td>MATLAB</td>
			<td>Version 2021b</td>
		</tr>
		<tr>
			<td>Processing Software</td>
			<td>Python Software Foundation</td>
			<td>Python</td>
			<td>Version 3.7.10</td>
		</tr>
	</tbody>
</table>

focused ultrasound neuromodulation of human in vitro neural cultures in multi-well microelectrode arrays

The neuromodulatory effects of focused ultrasound (FUS) have been demonstrated in animal models, and FUS has been used successfully to treat movement and psychiatric disorders in humans. However, despite the success of FUS, the mechanism underlying its effects&#160;on neurons remains poorly understood, making treatment optimization by tuning FUS parameters difficult. To address this gap in knowledge, we studied human neurons in vitro using neurons cultured from human-induced pluripotent stem cells (HiPSCs). Using HiPSCs allows for the study of human-specific neuronal behaviors in both physiologic and pathologic states. This report presents a protocol for using a high-throughput system that enables the monitoring and quantification of the neuromodulatory effects of FUS on HiPSC neurons. By varying the FUS parameters and manipulating the HiPSC neurons through pharmaceutical and genetic modifications, researchers can evaluate the neural responses and elucidate the neuro-modulatory effects of FUS on HiPSC neurons. This research could have significant implications for the development of safe and effective FUS-based therapies for a range of neurological and psychiatric disorders.

In summary, we present a protocol that enables in vitro FUS neuromodulation monitoring using neurons cultured from HiPSCs. The overall system platform to stimulate HiPSC-induced neurons and record the corresponding electrical responses for analysis is outlined in Figure 1. This study focuses on the FUS stimulation of neurons and recording the electrical responses in an MEA system, as shown in Figure 2. The peripheral components of the FUS and MEA systems and their connections are illustrated in Figure 3.
The characterization of the focal point is performed prior to the neuronal experiments to ensure the bottom of the well is fully covered by the FUS focal point. The visualization of the focal spot on thermochromic sheets, as shown in Figure 4, should be performed to evaluate the FUS system. Following focal spot characterization, the post-processing steps, including filtering, thresholding, and calculating the firing rate, should be performed, and these are summarized in Figure 5 and Figure 6. These steps are essential to retrieve useful signals by filtering noise from the environment and, thus, to gain insight into the neuronal activity changes caused by FUS. The Raster plots in Figure 6A-B show the detected spikes in each channel. As the entire bottom of the well is within the focal point of the FUS transducer, it is expected that the FUS should alter the firing rate across all the electrodes. This change in firing rate is visualized in the firing rate plot shown in Figure 6C, which shows that the chosen stimulation parameters resulted in an increase in the neuronal firing rate. Specifically, the pre-FUS (i.e., baseline) firing rate was 140 Hz &#177; 116.7 Hz, while the post-FUS firing rate was 786 Hz &#177; 419.4 Hz with continuous-wave FUS. Additionally, Figure 6C shows how altering the FUS parameters (e.g., using pulsed-wave FUS instead of continuous-wave) can alter the magnitude of change in the firing rate, as well as change the amount of time before the neurons return to their baseline state. Low-intensity focused ultrasound (LIFU) does not cause significant warming of cultures, especially when compared to high-intensity focused ultrasound, which intends to achieve thermal lesion. The lack of clinically impactful temperature change is supported by theoretical calculations and simulations (Supplementary Figure 2). Even in extreme cases of the experimental FUS parameters listed in Table 1, only a minimal increase in temperature could be observed of approximately 0.04 &#176;C.
The use of a firing rate plot enables the quantification of the neuromodulatory effects of FUS and can be used to differentiate between excitatory and inhibitory responses. A significant advantage of the multi-well MEA plate is that it can be reused multiple times to study varying neuronal states and stimulation parameters in a high-throughput manner.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/65115/65115fig01.jpg" /> 
Figure 1: Overview of the in vitro platform for the focused ultrasound (FUS) neuromodulation of neurons in a well and the measurement of their neuronal activity using a microelectrode array. Each electrode (red, green, and blue lines) records from a population of neurons within a single well. A processing pipeline is implemented to convert the raw neuronal electrical recordings into the detection of neuronal firing patterns. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig01large.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/65115/65115fig02.jpg" /> 
Figure 2: FUS neuromodulation with a multi-well microelectrode array (MEA). (A) Schematic of the setup for FUS neuromodulation with a multi-well MEA. The acoustic waves generated by the FUS transducer propagate through an FUS cone filled with degassed water and are coupled using ultrasound gel. The parafilm is secured to the well using a rubber band to prevent contamination. The MEA plate sends electrical recordings from the neurons to the MEA system. (B) A photograph of the FUS transducer on the multi-well plate contained in the MEA system. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig02large.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/65115/65115fig03.jpg" /> 
Figure 3: In vitro platform setup. (A) The front of the in vitro platform setup. The transducer power output (TPO; left) is used to program the FUS parameters. The MEA system (right) records electrical activity from the neurons in the well plate, which are neuromodulated by the FUS transducer. (B) The back of the in vitro platform setup with connections from the matching network (1) to the TPO and (2) to the transducer. (3) The connection from the MEA system to the TPO synchronizes the data acquisition. (4) The connection from the MEA system to the computer for data transfer. (5) The power connection to the MEA system. (6) The power connection to the FUS system. (7) The sonication button. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig03large.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/65115/65115fig04v2.jpg" /> 
Figure 4: Characterization of the FUS transducer. (A) A pressure map of the focal spot using the FUS parameters detailed in Table 1 measured by the AMPLITUDE system15. (B) Pre- and post-sonication of a thermochromic sheet placed at the bottom of a well using the experimental setup shown in Figure 3. The thermochromic sheet changes color in response to temperature changes, which provides a visual validation of successful stimulation at the location of the neurons. The maximal spatial-peak pulse average intensity (ISPPA) of 30 W/cm2 and continuous sonication of 3 min were adjusted to change the local temperature drastically for the better visualization of such a focal point. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig04largev2.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/65115/65115fig05.jpg" /> 
Figure 5: Processing pipeline. Step 1: Raw electrical recordings are captured from N = 16 channels. The future steps show the process using channel 16 (outlined in red). Step 2: For each channel, a Butterworth bandpass filter (5 Hz to 3 kHz bandpass) is applied, followed by a Gaussian filter (&#963; = 3). A threshold is set as five times the standard deviation of the signal within a 2 s window centered at the start of the sonication. Step 3: Signals above or below the threshold are characterized as spikes. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig05large.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/65115/65115fig06.jpg" /> 
Figure 6: Raster and firing rate plots. (A) Raster plot of the detected spikes at each channel as a function of the sonication time. The time of FUS stimulation is annotated using a red line. (B) Raster plot of neurons under different FUS settings with continuous FUS for comparison. (C) The firing rate was calculated using a 50 ms sliding window. The mean firing rates pre- and post FUS neuromodulations were 140 Hz and 786 Hz, respectively. With pulsed FUS, the mean firing rates were 230 Hz and 540 Hz. A shorter activation and less rate change were observed to be induced by this set of varying FUS stimulation. The process for calculating the firing rate is detailed in Supplementary Figure 1. <a href="https://www.jove.com/files/ftp_upload/65115/65115fig06large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Parameter</td>
			<td>Value</td>
		</tr>
		<tr>
			<td>Max Power/Ch.</td>
			<td>1.200 W</td>
		</tr>
		<tr>
			<td>Pactual</td>
			<td>0.749 W/channel.</td>
		</tr>
		<tr>
			<td>ISPPA</td>
			<td>10.79 W/cm2</td>
		</tr>
		<tr>
			<td>ISPTA</td>
			<td>0.05 W/cm2</td>
		</tr>
		<tr>
			<td>Burst Length</td>
			<td>0.100 ms</td>
		</tr>
		<tr>
			<td>Frequency</td>
			<td>250.00 kHz</td>
		</tr>
		<tr>
			<td>Focus</td>
			<td>39.800 mm</td>
		</tr>
		<tr>
			<td>Period</td>
			<td>20.000 ms</td>
		</tr>
		<tr>
			<td>Timer</td>
			<td>60.000 s</td>
		</tr>
	</tbody>
</table>
Table 1: Focused ultrasound (FUS) parameters set on the TPO for the study presented in Figure 4.
Supplementary Figure 1: Processing from the Raster plot to the firing rate. Step 1: Count the spikes among all the channels to obtain the count number within a given sliding window. Note: Here, a larger sliding window (set to 0.1 s) was chosen for better illustration. Step 2: Convert the spikes per window length to spikes per second (e.g., here, multiply the counts by 10 to convert to hertz [Hz], and then divide by 1,000 to obtain the value in kilohertz [kHz]). Step 3: The firing rate curve acquired as a result. An open-source toolkit, along with sampled data, is available on GitHub (https://github.com/Rxliang/FUSNeuromod). <a href="https://www.jove.com/files/ftp_upload/65115/SupFig1.pdf" target="_blank">Please click here to download this File.</a>
Supplementary Figure 2: K-wave simulation result temperature profile of LIFU16. Based on the acoustic intensity map shown in Figure 4, the K-wave simulation result suggests a maximal temperature increase of 0.04 &#176;C within the center region of the focal zone (radius: 2 mm) using the extreme case of the experimental FUS parameters listed in Table 1. <a href="https://www.jove.com/files/ftp_upload/65115/SupFig2.pdf" target="_blank">Please click here to download this File.</a>

Watch this Scientific Journal Video about Focused Ultrasound Neuromodulation of Human In Vitro Neural Cultures in Multi-Well Microelectrode Arrays at JoVE.com

Focused Ultrasound Neuromodulation of Human In Vitro Neural Cultures in Multi-Well Microelectrode Arrays

Here, we present a protocol for using a high-throughput system that enables the monitoring and quantification of the neuromodulatory effects of focused ultrasound on human-induced pluripotent stem cell (HiPSC) neurons.

Focused Ultrasound Neuromodulation of Human In Vitro Neural Cultures in Multi-Well Microelectrode Arrays

The neuromodulatory effects of focused ultrasound (FUS) have been demonstrated in animal models, and FUS has been used successfully to treat movement and ...

focused-ultrasound-neuromodulation-human-vitro-neural-cultures-multi

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Research

JoVE Journal

Neuroscience

Time-lapse Live Imaging of Clonally Related Neural Progenitor Cells in the Developing Zebrafish Forebrain

Precise patterns of division, migration and differentiation of neural progenitor cells are crucial for proper brain development and function1,2. To understand the behavior of neural progenitor cells in the complex in vivo environment, time-lapse live imaging of neural progenitor cells in an intact brain is critically required. In this video, we exploit the unique features of zebrafish embryos to visualize the development of forebrain neural progenitor cells in vivo. We use electroporation to genetically and sparsely label individual neural progenitor cells. Briefly, DNA constructs coding for fluorescent markers were injected into the forebrain ventricle of 22 hours post fertilization (hpf) zebrafish embryos and electric pulses were delivered immediately. Six hours later, the electroporated zebrafish embryos were mounted with low melting point agarose in glass bottom culture dishes. Fluorescently labeled neural progenitor cells were then imaged for 36hours with fixed intervals under a confocal microscope using water dipping objective lens. The present method provides a way to gain insights into the in vivo development of forebrain neural progenitor cells and can be applied to other parts of the central nervous system of the zebrafish embryo.

The present video demonstrates a method which takes advantage of the combination of electroporation and confocal microscopy to perform live imaging on individual neural progenitor cells in the developing zebrafish forebrain. In vivo analysis of the development of forebrain neural progenitor cells at a clonal level can be achieved in this way.

Precise patterns of division, migration and differentiation of neural progenitor cells are crucial for proper brain development and function1,2. To ...

Interfacing 3D Engineered Neuronal Cultures to Micro-Electrode Arrays: An Innovative In Vitro Experimental Model

Currently, large-scale networks derived from dissociated neurons growing and developing in vitro on extracellular micro-transducer devices are the gold-standard experimental model to study basic neurophysiological mechanisms involved in the formation and maintenance of neuronal cell assemblies. However, in vitro studies have been limited to the recording of the electrophysiological activity generated by bi-dimensional (2D) neural networks. Nonetheless, given the intricate relationship between structure and dynamics, a significant improvement is necessary to investigate the formation and the developing dynamics of three-dimensional (3D) networks. In this work, a novel experimental platform in which 3D hippocampal or cortical networks are coupled to planar Micro-Electrode Arrays (MEAs) is presented. 3D networks are realized by seeding neurons in a scaffold constituted of glass microbeads (30-40 &#181;m in diameter) on which neurons are able to grow and form complex interconnected 3D assemblies. In this way, it is possible to design engineered 3D networks made up of 5-8 layers with an expected final cell density. The increasing complexity in the morphological organization of the 3D assembly induces an enhancement of the electrophysiological patterns displayed by this type of networks. Compared with the standard 2D networks, where highly stereotyped bursting activity emerges, the 3D structure alters the bursting activity in terms of duration and frequency, as well as it allows observation of more random spiking activity. In this sense, the developed 3D model more closely resembles in vivo neural networks.

Interfacing 3D Engineered Neuronal Cultures to Micro-Electrode Arrays: An Innovative In Vitro Experimental Model

In this work, a novel experimental model in which 3D neuronal cultures are coupled to planar Micro-Electrode Arrays (MEAs) is presented. 3D networks are built by seeding neurons in a scaffold made up of glass microbeads on which neurons grow and form interconnected 3D structures.

Currently, large-scale networks derived from dissociated neurons growing and developing in vitro on extracellular micro-transducer devices are the ...

Time-dependent Increase in the Network Response to the Stimulation of Neuronal Cell Cultures on Micro-electrode Arrays

Micro-electrode arrays (MEAs) can be used to investigate drug toxicity, design paradigms for next-generation personalized medicine, and study network dynamics in neuronal cultures. In contrast with more traditional methods, such as patch-clamping, which can only record activity from a single cell, MEAs can record simultaneously from multiple sites in a network, without requiring the arduous task of placing each electrode individually. Moreover, numerous control and stimulation configurations can be easily applied within the same experimental setup, allowing for a broad range of dynamics to be explored. One of the key dynamics of interest in these in vitro studies has been the extent to which cultured networks display properties indicative of learning. Mouse neuronal cells cultured on MEAs display an increase in response following training induced by electrical stimulation. This protocol demonstrates how to culture neuronal cells on MEAs; successfully record from over 95% of the plated dishes; establish a protocol to train the networks to respond to patterns of stimulation; and sort, plot, and interpret the results from such experiments. The use of a proprietary system for stimulating and recording neuronal cultures is demonstrated. Software packages are also used to sort neuronal units. A custom-designed graphical user interface is used to visualize post-stimulus time histograms, inter-burst intervals, and burst duration, as well as to compare the cellular response to stimulation before and after a training protocol. Finally, representative results and future directions of this research effort are discussed.

Mouse neuronal cells cultured on multi-electrode arrays display an increase in response following electrical stimulation. This protocol demonstrates how to culture neurons, how to record activity, and how to establish a protocol to train the networks to respond to patterns of stimulation.

Micro-electrode arrays (MEAs) can be used to investigate drug toxicity, design paradigms for next-generation personalized medicine, and study network ...

Recording and Modulation of Epileptiform Activity in Rodent Brain Slices Coupled to Microelectrode Arrays

Temporal lobe epilepsy (TLE) is the most common partial complex epileptic syndrome and the least responsive to medications. Deep brain stimulation (DBS) is a promising approach when pharmacological treatment fails or neurosurgery is not recommended. Acute brain slices coupled to microelectrode arrays (MEAs) represent a valuable tool to study neuronal network interactions and their modulation by electrical stimulation. As compared to conventional extracellular recording techniques, they provide the added advantages of a greater number of observation points and a known inter-electrode distance, which allow studying the propagation path and speed of electrophysiological signals. However, tissue oxygenation may be greatly impaired during MEA recording, requiring a high perfusion rate, which comes at the cost of decreased signal-to-noise ratio and higher oscillations in the experimental temperature. Electrical stimulation further stresses the brain tissue, making it difficult to pursue prolonged recording/stimulation epochs. Moreover, electrical modulation of brain slice activity needs to target specific structures/pathways within the brain slice, requiring that electrode mapping be easily and quickly performed live during the experiment. Here, we illustrate how to perform the recording and electrical modulation of 4-aminopyridine (4AP)-induced epileptiform activity in rodent brain slices using planar MEAs. We show that the brain tissue obtained from mice outperforms rat brain tissue and is thus better suited for MEA experiments. This protocol guarantees the generation and maintenance of a stable epileptiform pattern that faithfully reproduces the electrophysiological features observed with conventional field potential recording, persists for several hours, and outlasts sustained electrical stimulation for prolonged epochs. Tissue viability throughout the experiment is achieved thanks to the use of a small-volume custom recording chamber allowing for laminar flow and quick solution exchange even at low (1 mL/min) perfusion rates. Quick MEA mapping for real-time monitoring and selection of stimulating electrodes is performed by a custom graphic user interface (GUI).

We illustrate how to perform recording and electrical modulation of 4-aminopyridine-induced epileptiform activity in rodent brain slices using microelectrode arrays. A custom recording chamber maintains tissue viability throughout prolonged experimental sessions. Live electrode mapping and selection of stimulating pairs are performed by a custom graphical user interface.

Temporal lobe epilepsy (TLE) is the most common partial complex epileptic syndrome and the least responsive to medications. Deep brain stimulation (DBS) ...

Stereotaxic Surgery for Implantation of Microelectrode Arrays in the Common Marmoset (Callithrix jacchus)

Marmosets (Callithrix jacchus) are small non-human primates that are gaining popularity in biomedical and preclinical research, including the neurosciences. Phylogenetically, these animals are much closer to humans than rodents. They also display complex behaviors, including a wide range of vocalizations and social interactions. Here, an effective stereotaxic neurosurgical procedure for implantation of recording electrode arrays in the common marmoset is described. This protocol also details the pre- and postoperative steps of animal care that are required to successfully perform such a surgery. Finally, this protocol shows an example of local field potential and spike activity recordings in a freely behaving marmoset 1 week after the surgical procedure. Overall, this method provides an opportunity to study the brain function in awake and freely behaving marmosets. The same protocol can be readily used by researchers working with other small primates. In addition, it can be easily modified to allow other studies requiring implants, such as stimulating electrodes, microinjections, implantation of optrodes or guide cannulas, or ablation of discrete tissue regions.

Stereotaxic Surgery for Implantation of Microelectrode Arrays in the Common Marmoset Callithrix jacchus

This work presents a protocol to perform a stereotaxic, neurosurgical implantation of&#160;microelectrode arrays in the common marmoset. This method specifically enables electrophysiological recordings in freely behaving animals but can be easily adapted to any other similar neurosurgical intervention in this species (e.g., cannula for drug administration or electrodes for brain stimulation).

Marmosets (Callithrix jacchus) are small non-human primates that are gaining popularity in biomedical and preclinical research, including the ...

Focused Ultrasound Induced Blood-Brain Barrier Opening for Targeting Brain Structures and Evaluating Chemogenetic Neuromodulation

Acoustically Targeted Chemogenetics (ATAC) allows for the noninvasive control of specific neural circuits. ATAC achieves such control through a combination of focused ultrasound (FUS) induced blood-brain barrier opening (FUS-BBBO), gene delivery with adeno-associated viral (AAV) vectors, and activation of cellular signaling with engineered, chemogenetic, protein receptors and their cognate ligands. With ATAC, it is possible to transduce both large and small brain regions with millimeter precision using a single noninvasive ultrasound application. This transduction can later allow for a long-term, noninvasive, device-free neuromodulation in freely moving animals using a drug. Since FUS-BBBO, AAVs, and chemogenetics have been used in multiple animals, ATAC should also be scalable for the use in other animal species. This paper expands upon a previously published protocol and outlines how to optimize the gene delivery with FUS-BBBO to small brain regions with MRI-guidance but without a need for a complicated MRI-compatible FUS device. The protocol, also, describes the design of mouse targeting and restraint components that can be 3D-printed by any lab and can be easily modified for different species or custom equipment. To aid reproducibility, the protocol describes in detail how the microbubbles, AAVs, and venipuncture were used in ATAC development. Finally, an example data is shown to guide the preliminary investigations of studies utilizing ATAC.

This protocol delineates steps necessary for the gene delivery through focused ultrasound blood brain barrier (BBB) opening, evaluation of the resulting gene expression, and measurement of neuromodulation activity of chemogenetic receptors through histological tests.

Acoustically Targeted Chemogenetics (ATAC) allows for the noninvasive control of specific neural circuits. ATAC achieves such control through a ...

Delivery of Antibodies into the Brain Using Focused Scanning Ultrasound

Only a small fraction of therapeutic antibodies targeting brain diseases are taken up by the brain. Focused ultrasound offers a possibility to increase uptake of antibodies and engagement through transient opening of the blood-brain barrier (BBB). In our laboratory, we are developing therapeutic approaches for neurodegenerative diseases in which an antibody in various formats is delivered across the BBB using microbubbles, concomitant with focused ultrasound application through the skull targeting multiple spots, an approach we refer to as scanning ultrasound (SUS). The mechanical effects of microbubbles and ultrasound on blood vessels increases paracellular transport across the BBB by transiently separating tight junctions and enhances vesicle- mediated transcytosis, allowing antibodies and therapeutic agents to effectively cross. Moreover, ultrasound also facilitates the uptake of antibodies from the interstitial brain into brain cells such as neurons where the antibody distributes throughout the cell body and even into neuritic processes. In our studies, fluorescently labeled antibodies are prepared, mixed with in-house prepared lipid-based microbubbles and injected into mice immediately before SUS is applied to the brain. The increased antibody concentration in the brain is then quantified. To account for alterations in normal brain homeostasis, microglial phagocytosis can be used as a cellular marker. The generated data suggest that ultrasound delivery of antibodies is an attractive approach to treat neurodegenerative diseases.

Presented here is a protocol to transiently open the blood-brain barrier (BBB) either focally or throughout a mouse brain to deliver fluorescently-labeled antibodies and activate microglia. Also presented is a method to detect the delivery of antibodies and microglia activation by histology.

Only a small fraction of therapeutic antibodies targeting brain diseases are taken up by the brain. Focused ultrasound offers a possibility to increase ...

Construction and Implementation of Carbon Fiber Microelectrode Arrays for Chronic and Acute In Vivo Recordings

Multichannel electrode arrays offer insight into the working brain and serve to elucidate neural processes at the single-cell and circuit levels. Development of these tools is crucial for understanding complex behaviors and cognition and for advancing clinical applications. However, it remains a challenge to densely record from cell populations stably and continuously over long time periods. Many popular electrodes, such as tetrodes and silicon arrays, feature large cross-diameters that produce damage upon insertion and elicit chronic reactive tissue responses associated with neuronal death, hindering the recording of stable, continuous neural activity. In addition, most wire bundles exhibit broad spacing between channels, precluding simultaneous recording from a large number of cells clustered in a small area. The carbon fiber microelectrode arrays described in this protocol offer an accessible solution to these concerns. The study provides a detailed method for fabricating carbon fiber microelectrode arrays that can be used for both acute and chronic recordings in vivo. The physical properties of these electrodes make them ideal for stable and continuous long-term recordings at high cell densities, enabling the researcher to make robust, unambiguous recordings from single units across months.

Construction and Implementation of Carbon Fiber Microelectrode Arrays for Chronic and Acute In Vivo Recordings

This protocol describes a procedure for constructing carbon fiber microelectrode arrays for chronic and acute in vivo electrophysiological recordings in mouse (Mus musculus) and ferret (Mustela putorius furo) from multiple brain regions. Each step, following the purchase of raw carbon fibers to microelectrode array implantation, is described in detail, with emphasis on microelectrode array construction.

Multichannel electrode arrays offer insight into the working brain and serve to elucidate neural processes at the single-cell and circuit levels. ...

Recording Network Activity in Spinal Nociceptive Circuits Using Microelectrode Arrays

The roles and connectivity of specific types of neurons within the spinal cord dorsal horn (DH) are being delineated at a rapid rate to provide an increasingly detailed view of the circuits underpinning spinal pain processing. However, the effects of these connections for broader network activity in the DH remain less well understood because most studies focus on the activity of single neurons and small microcircuits. Alternatively, the use of microelectrode arrays (MEAs), which can monitor electrical activity across many cells, provides high spatial and temporal resolution of neural activity. Here, the use of MEAs with mouse spinal cord slices to study DH activity induced by chemically stimulating DH circuits with 4-aminopyridine (4-AP) is described. The resulting rhythmic activity is restricted to the superficial DH, stable over time, blocked by tetrodotoxin, and can be investigated in different slice orientations. Together, this preparation provides a platform to investigate DH circuit activity in tissue from na&#239;ve animals, animal models of chronic pain, and mice with genetically altered nociceptive function. Furthermore, MEA recordings in 4-AP-stimulated spinal cord slices can be used as a rapid screening tool to assess the capacity of novel antinociceptive compounds to disrupt activity in the spinal cord DH.

The combined use of microelectrode array technology and 4-aminopyridine-induced chemical stimulation for investigating network-level nociceptive activity in the spinal cord dorsal horn is outlined.