This work was funded by the National Institutes of Health National Institute of Allergy and Infectious Diseases (IAA number AOD12058-0001-0000) and the Defense Threat Reduction Agency &#8211; Joint Science and Technology Office, Medical S&#38;T Division (grant numbers CBM.THRTOX.01.10.RC.023 and CBM.THRTOX.01.RC.014). This research was performed while P.B. held a Defense Threat Reduction Agency-National Research Council Research Associateship Award and K.H. held a National Research Council Research Associateship Award. We thank Angela Adkins and Kaylie Tuznik (USAMRICD) for technical assistance; and Cindy Kronman (USAMRICD) for editorial assistance. The views expressed in this article are those of the authors and do not reflect the official policy of the Department of Army, Department of Defense, or the U.S. Government.

1. Adaptation of ESCs to Feeder Cell-free Suspension Culture
<ol>
	<li>Thaw ESCs at 37 &#176;C until a sliver of ice remains.</li>
	<li>Using a P1000 pipet, gently transfer 1 - 2.5 x 106 dissociated ESCs to a non-tissue culture-treated dish containing 10 ml of pre-warmed ESC medium. Incubate in a humidified tissue culture incubator for 20 hr at 37 &#176;C and 5% CO2.</li>
	<li>After 20 hr, wash cells by gently transferring the suspension culture to a 15 ml conical tube using a 10 ml serological pipet. Pellet ESCs for 3 min at 200 x g. During spin, add 10 ml of fresh ESC medium back to low-adhesion dish.</li>
	<li>Aspirate supernatant, taking care to avoid dislodging the cell pellet, and add 1 ml fresh ESC medium to cell pellet. Transfer cells to the bacterial dish using a P1000 pipet and return to the incubator.</li>
	<li>Observe cells daily until aggregates become visible to the naked eye (typically 4 - 8 days (d); aggregates will be 0.2 - 0.5 mm). If aggregates are not apparent after 4 d, repeat step 1.3. Once aggregates are visible, dissociate and maintain ESCs as described in Section 2.</li>
</ol>
2. ESC Passaging and Maintenance
<ol>
	<li>Transfer ESC aggregates to a 15 ml conical tube using a sterile 10 ml pipet and allow aggregates to settle to a compact pellet (typically 3 - 5 min). Aspirate the supernatant, being careful to avoid disrupting the cell pellet, and wash aggregates with 5 ml PBS. Although gravity settling is recommended, alternatively pellet cells at 100 x g for 2.5 min instead to save time.</li>
	<li>Aspirate PBS and add 500 &#181;l trypsin. Incubate aggregates in trypsin for 3 min in a water bath at 37 &#176;C. Add 500 &#181;l ESC medium to dilute the trypsin and gently triturate 10 times with a P1000 pipet to break up aggregates. Count cells using a hemocytometer.</li>
	<li>Pellet dissociated cells for 3 min at 200 x g and resuspend cells to a final concentration of 1.0 x 107 cells/ml in ESC medium. Transfer 150 &#181;l (1.5 x 106 cells) to 10 ml of fresh ESC medium in a 10 cm bacterial dish and return to tissue culture incubator for 48 hr. Excess ESCs can be differentiated, cryopreserved at 1 - 5 x 106 cells/ml in 90% ESC medium supplemented with 10% DMSO, or discarded.</li>
	<li>Passage aggregates every 48 hr. Aggregates ready for passage will be clearly visible, with diameters exceeding 0.5 mm. 
	NOTE: Thawing and culture of cryopreserved, suspension-adapted cells are accomplished per steps 1.2 - 1.4. Aggregates will be ready for passaging within 48 - 72 hr.</li>
</ol>
3. Neuronal Differentiation
NOTE: Conduct steps 3.1 - 3.5 prior to noon and step 3.7 after noon. An overview of the differentiation procedures is presented in Figure 1A.
<ol>
	<li>Dissociate ESCs as in steps 2.1 - 2.5. Transfer 350 &#181;l (3.5 x 106) of dissociated ESCs to a 10 cm low-attachment dish containing 25 ml differentiation medium. Place on an orbital shaker set to 30 - 45 rpm inside a tissue culture incubator at 37 &#176;C with 5% CO2. This is the first day of differentiation, termed day in vitro (DIV) -8. 
	NOTE: The use of an ultra-low attachment dish increases the cost of the method, but produces slightly larger yields than bacterial Petri dishes since aggregates can occasionally adhere to Petri dishes. If different dish sizes are preferred, medium volumes and cell numbers can be scaled accordingly.</li>
	<li>After 48 hr (DIV -6), use a 25 ml pipet to transfer the differentiating cell aggregates to a 50 ml conical tube. Immediately add a fresh 25 ml of differentiation medium to the Petri dish.</li>
	<li>Allow aggregates to settle over 2 - 5 min, producing a visible pellet that is 1 - 2 mm deep. Ignore single cells or small aggregates remaining in suspension. Carefully aspirate the medium and transfer the cell pellet back to the petri dish using a P1000. Place on rotary shaker in a tissue culture incubator.</li>
	<li>At DIV -4 repeat step 3.2. The pellet will be 2 - 4 mm deep. Replace 30 ml differentiation medium supplemented with 6 &#181;M all-trans retinoic acid (RA) to the petri dish. Return to rotary shaker in the tissue culture incubator for an additional 48 hr.</li>
	<li>At DIV -2 repeat step 3.3. The pellet will be 4 - 8 mm deep at this point.</li>
	<li>At DIV -1, prepare plating surfaces as in Section 4.</li>
	<li>At DIV 0, thaw 5 ml of pre-aliquoted and frozen NPC trypsinization medium at 37 &#176;C for 5 - 10 min and place in a tissue culture hood. Using a 25 ml pipet, transfer differentiating aggregates to a 50 ml conical tube. Allow aggregates to settle and carefully aspirate medium. Wash pellet twice with 10 ml PBS, allowing the aggregates to settle between washes.</li>
	<li>After the second PBS wash, add 5 ml of NPC trypsinization medium to the pellet and incubate at 37 &#176;C for 5 min. Gently flick the tube after 2.5 min.</li>
	<li>Add 5 ml of 0.1% soybean trypsin inhibitor (STI) to inactivate trypsin and mix by inverting. Gently triturate 10 - 15 times with a 10 ml serological pipet until a relatively homogenous cell suspension is produced.</li>
	<li>Slowly transfer the cell suspension to a 40 &#181;m or 70 &#181;m cell strainer placed in the top of a 50 ml conical tube. Once all the suspension has been filtered, add 1 ml of N2 medium to wash remaining cells through the filter and pellet the dissociated cell suspension for 6 min at 200 x g.</li>
	<li>Aspirate medium without disturbing the pellet. Wash cells twice with 10 ml N2 medium, pelleting cells for 5 min at 200 x g and triturating between washes with a P1000. Prior to the second wash, count cells using a hemocytometer.</li>
	<li>Resuspend cells in N2 medium at 1 x 107 cells per ml and plate ESNs at a cell density of 150,000 - 200,000 cells/cm2.</li>
	<li>Transfer newly plated ESNs to a humidified tissue culture incubator at 37 &#176;C and 5% CO2 and maintain as in Section 5.</li>
</ol>
4. Preparing Culture Surfaces for Plating Neural Precursors at DIV 0
<ol>
	<li>Prepare tissue culture-treated dishes at least 1 day prior to plating. Add sufficient polyethyleneimine (PEI; 25 &#181;g/ml in sterile H2O) or poly-D-lysine (PDL; 100 &#181;g/ml in sterile H2O) to cover tissue-culture-treated plastic dishes and incubate O/N at 37 &#176;C.</li>
	<li>The morning of plating, wash dishes twice with double-distilled H2O and once with PBS. After the final wash, add sufficient N2 medium to cover the dish (e.g., 1 ml per well of a 12-well dish or 4 ml per 6 cm dish).</li>
	<li>Prepare 18 mm glass coverslips at least one day prior to neuron plating. Clean coverslips by plasma-cleaning for 4 min.</li>
	<li>Immediately transfer cleaned coverslips to an ethanol-washed parafilm in the bottom of a large sterile dish and add 400 &#181;l of PEI or PDL solution, prepared as in step 4.1. Incubate O/N at 37 &#176;C in a tissue culture incubator.</li>
	<li>In the morning, wash coverslips three times with water and add 5 &#181;g/ml laminin in PBS for 1 - 3 hr at 37 &#176;C. Prior to dissociating neurons, aspirate the laminin and immediately transfer the coverslip to a well of a 12-well dish containing 1 ml of NPC medium, being sure to keep the treated side facing up.</li>
	<li>Store dishes and coverslips at 37 &#176;C until NPCs are ready to plate.</li>
</ol>
5. Maintenance of Neurons
<ol>
	<li>At DIV 1, aspirate medium and replace with N2 culture medium.</li>
	<li>At DIV 2 and 4, aspirate medium and replace with B27 culture medium.</li>
	<li>At DIV 8, aspirate medium and replace with B27 culture medium containing mitotic inhibitors to eliminate contaminating non-neuronal cells.</li>
	<li>At DIV 12, replace with B27 culture medium.</li>
	<li>Do not remove DIV 12+ ESNs from 5% CO2 until ready to use.</li>
</ol>
6. Measured Inhibition of Synaptic Transmission (MIST) Assay for Quantifying Miniature Excitatory Post-synaptic Currents
CAUTION: The Clostridial neurotoxins are the most poisonous substances known, with estimated human LD50 values as low as 0.1 - 1 ng/kg. Obtain necessary approvals prior to using these toxins and use appropriate precautions.
<ol>
	<li>Carefully dilute BoNT/A to 100x the desired final concentration in ESN culture medium and warm to 37 &#186;C. Add appropriate volume of toxin to DIV 21+ ESN cultures, swirl the culture dish, and return to incubator.</li>
	<li>If cells will be analyzed more than 4 hr after intoxication, add toxin to the dish and swirl without removing from 5% CO2, such as directly in the incubator or in a constant CO2 chamber.</li>
	<li>At appropriate time point, aspirate ESN culture medium and wash twice with extracellular recording buffer (ERB). Add 4 ml of ERB supplemented with 5.0 &#181;M tetrodotoxin and 10 &#181;M bicuculline, blocking action potentials and antagonizing GABAA receptor activity, respectively.</li>
	<li>Transfer dish to electrophysiology rig. Neither perfusion nor temperature control is required for the MIST assay.</li>
	<li>Pull borosilicate glass using a micropipette puller to produce a recording pipette with 5-10 m&#937; of resistance and fill with intracellular recording buffer. Gently dip filled recording pipette in siliconizing reagent prior to recording.</li>
	<li>Using an air-filled syringe, provide positive pressure as the recording pipette is lowered into the ERB. After gently landing the recording pipette on the soma of the neuron to be recorded, remove positive pressure and form a gigaseal. Decrease the holding voltage to -70 mV. Carefully apply negative pressure to break into whole-cell configuration.</li>
	<li>Switch to current-clamp to monitor and record resting membrane potential. Without adjustment for liquid junction potentials, the resting membrane potential will be between -67 to -82 mV.</li>
	<li>Perform a continuous -70 mV voltage-clamp recording for 4 - 5 min to detect miniature excitatory post-synaptic currents (mEPSCs).</li>
	<li>Analyze 4 min of recorded data for mEPSC detection using spike detection software with the following settings: Threshold, 5; Period to search a local maximum, 10,000 &#181;sec; Time before a peak for baseline, 5,000 &#181;sec; Period to search a decay time, 20,000 &#181;sec; Fraction of peak to find a decay time, 0.37; Period to average a baseline, 1,000 &#181;sec; Area threshold, 20; Number of points to average peak, 1; Direction of peak, negative.</li>
	<li>Collect and save information on detected events. Divide the number of detected events in 4 min by 240 to determine the mEPSC frequency in Hz.</li>
	<li>Collect mEPSC frequencies for 8 - 12 controls and 8 - 12 BoNT-treated samples for each exposure condition. Analyze frequency against age- and lot-matched controls. Determine the statistical significance of % inhibition of synaptic activity using one-way ANOVA testing and Dunnett&#8217;s post-hoc test.</li>
</ol>

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The U.S. Government has filed two international patent applications that incorporate methods described in this article: PCT/US2014/22042, titled &#8220;Methods of detecting neurotoxin using synaptic activity&#8221;; and PCT/US13/40641, titled &#8220;Toxin detection using stem cell-derived neurons.&#8221;

The current gold standard for CNT detection, serotype determination and quantitation is the MLA. The MLA interrogates the entire range of host:toxin interactions required for intoxication to occur in vivo (e.g., toxin binding to a cell surface receptor, internalization of the toxin-receptor complex, LC translocation into the cytoplasm, LC-mediated cleavage of substrate and inhibition of synaptic neurotransmission)18. However, although the MLA offers a physiologically relevant model of intoxication, it is resource intensive, can be confounded by contaminants and involves large numbers of mice with death as an endpoint. Alternatively, cell-based assays for BoNT detection and quantitation have been limited to primary neuron cultures, which also require animal use, or to neuroblastoma cell lines, which fail to form synapses and typically exhibit poor sensitivity to neurotoxins8. To date, most measurements of intoxication in these cell-based platforms have relied on detection of the proteolytic cleavage of SNAP-25, VAMP1/2 or syntaxin-1 11. This is problematic because SNARE protein cleavage has been shown to be non-linearly associated with synaptic inhibition in vivo and therefore may not accurately represent intoxication or recovery from intoxication19,20.
An ideal cell-based model system for CNT detection would (i) be neuron-based; (ii) be synaptically coupled with neurotypic electrical responses; (iii) be highly sensitive to all CNT serotypes or subtypes; and (iv) offer scalability, throughput and assay times that are equivalent to or improved over the MLA, at lower cost, and without requiring animal use. To meet these requirements, we developed a method to produce large quantities of highly enriched, networked cultures of glutamatergic and GABAergic neurons from commercially available mouse ESC lines. We then developed the MIST assay to quantify synaptic inhibition in response to intoxication with TeNT and BoNT/A-/G. While the MIST assay can be conducted on any synaptically active neuron population (e.g., primary neurons or brain slices), currently ESNs are the only in vitro derived neuron model that reproducibly develops emergent network behaviors and is therefore appropriate for the MIST assay.
Producing sufficient quantities of neurons of defined lineage for CNT studies required several innovations in ESC culture and differentiation. First, by selecting for and culturing ESCs that can survive suspension-adaptation, we eliminated the potential for contamination by feeder cells and the need to purify feeder cells from ESCs at the start of differentiation. Although the molecular mechanisms underlying suspension-adaptation are unknown, suspension-adapted ESCs remain mitotically active, retain Oct3/4 expression and continue to be neurogenic. Using this method, ~1.5 x 107 ESCs are typically recovered each passage. Second, the production of NPCs was increased ~300% by incorporating mechanical agitation to prevent agglomeration during differentiation, ostensibly increasing nutrient accessibility to the interiors of aggregates. During the process, we found that the serum used for ESC culture and neuronal differentiation is the most critical component in maintaining neurogenic ESCs. For best success, we recommend suspension adapting ES cells to each lot of serum and stockpiling serum at -20 &#176;C to support ESC culture and neuronal differentiation through the expiration date.
As with most synaptically active cultures, DIV 14+ ESNs are highly susceptible to abrupt changes in pH, and even a brief exposure to atmospheric CO2 concentrations can result in neurotoxicity within 24 hr. For experiments requiring treatment of cultures followed by incubations lasting O/N or longer, neurons should be treated directly in the incubator or transferred to a constant CO2 chamber prior to experimentation.
A variety of techniques confirmed neurogenesis and neuronal maturation, including ICC, transcriptional profiling and whole-cell patch-clamp electrophysiology. Temporal changes in gene expression and neuron morphology were consistent with a rapid progression through the developmental stages of neurogenesis, and by DIV 16, ESNs exhibited excitatory and inhibitory miniature post-synaptic currents with emergent network behaviors16. Evidence of synaptic activity suggested that ESNs may replicate the pathophysiologies responsible for the clinical manifestations of botulism and tetanus. This was confirmed by using MIST to show that intoxication with BoNT/A-/G or TeNT impaired mEPSC frequencies by &#62;95% compared to vehicle-treated or untreated neurons.
Measurements of the sensitivity of MIST for BoNT/A indicated a median inhibitory concentration (IC50) of 0.013 pM (equivalent to 0.5 mouse lethal units/ml) and a limit-of-detection below 0.005 pM, measured at 20 hr after bath addition. Based on these values, MIST is approximately twice as sensitive as and 2 - 4 times faster than the MLA and 30-fold more sensitive than immunoblot-based detection of cleaved SNAP-25.
Collectively, these data suggest that networked populations of stem cell-derived neurons offer a physiologically relevant, cell-based model of intoxication. In combination with improved methods to derive networked ESN cultures from suspension-adapted ESCs, the use of MIST should reduce the need for animal testing and the associated disadvantages, costs and ethical concerns of the MLA while providing a more rapid, sensitive and specific measure of intoxication. Although whole-cell patch-clamp electrophysiology is a low-throughput method for identifying the presence of active neurotoxins, it offers a resolution and speed that is unachievable using molecular methods. These findings also provide evidence that the application of activity-dependent methods to evaluate synaptic activity and network behavior may enable the rapid and specific detection of neurotoxins. Such higher-throughput approaches would make mechanistic studies, therapeutic screening or diagnostic assays feasible for a wide array of neuromodulatory agents, including the CNTs.

The overall goal of this method is to functionally evaluate synaptic activity in networked cultures of stem cell-derived neurons exposed to clostridial neurotoxins. This is the first demonstration of an in vitro derived model that functionally replicates the pathophysiologies responsible for clinical manifestations of botulism and validates ESNs as a suitable model for detection of CNTs, therapeutic screening and mechanistic studies.
BoNTs are highly lethal bacterial neurotoxins produced by members of the Clostridium species. Including the recently proposed BoNT/H, eight antigenically distinct BoNT serotypes have been described (/A-/H)1,2. All serotypes are expressed as 150 kDa peptides that are post-translationally nicked to produce a dichain composed of a 100 kDa heavy chain (HC) and a 50 kDa light chain (LC) linked by a disulfide bond3. The HC mediates binding to presynaptic receptors and entry of the toxin into the neuron via synaptic endocytosis. During endosomal processing, the HC undergoes structural re-organization to form a pore in the vesicle membrane, facilitating the translocation of the LC into the presynaptic cytosol. The LC then specifically targets and cleaves soluble N-ethylmaleimide-sensitive fusion attachment protein receptor (SNARE) proteins in the presynaptic compartment: SNAP-25 (BoNT/A, /C, /E), VAMP2 (BoNT /B, /D, /F, /G) or syntaxin (BoNT/C)1. Cleavage of any of these SNARE proteins prevents the assembly of the synaptic exocytosis machinery, thereby blocking neurotransmitter release. This combination of efficient neuronal targeting and presynaptic localization renders BoNTs the most potent poisons known, with estimated human lethal doses as low as 0.1 - 1 ng/kg1.
Biochemical assays can be used to detect the presence or activity of CNT LCs with high sensitivity. However, these methods fail to interrogate the ability of the toxin to bind, enter, activate and function within neurons, and therefore are indirect and possibly misleading measures of the presence of active toxin. In contrast, functional assays of intoxication such as the mouse lethality assay (MLA) comprehensively evaluate the ability of CNTs to successfully negotiate all phases of uptake and activation, providing more relevant and specific assessments of toxin activity. While the MLA is the gold-standard of BoNT detection, it is an in vivo method that uses death as an end-point and therefore has limited utility as a research platform. Attempts to develop cell-based models of CNT intoxication suitable for mechanistic studies and therapeutic screening have also suffered significant limitations. While primary neuron cultures offer a high degree of physiological relevance, their use is complicated by a number of factors, including high resource cost, relatively low yield, the presence of multiple neuronal subtypes and extensive regulatory and administrative oversight involved with animal use. As an alternative to primary neurons, neurogenic cell lines (which can be induced to adopt neuron-like properties by chemical stimulation) such as neuroblastomas and adrenal chromaffin cells have been used as in vitro models of intoxication. Since these cells are continuously cultured prior to induction, they are highly scalable and therefore well-suited for moderate-throughput approaches. However, their relevance is questionable since induced phenotypes are typically heterogeneous, are poorly sensitive to CNTs and fail to exhibit critical neuronal behaviors, including the inability to form pre- and post-synaptic compartments that assemble into functioning synapses4. In the absence of physiologically intact presynaptic compartments, the full range of toxin:neuron interactions cannot be replicated and therefore functional measurements of intoxication are not possible5. Not surprisingly, attempts to conduct mechanistic studies or drug screening for BoNTs using induced neurogenic cell lines have resulted in findings that are inconsistent with in vivo and primary neuron studies6.
It has been proposed that stem cell-derived central nervous system (CNS) neurons may provide a next-generation cell-based platform for BoNT research that combines the relevance of primary neurons with the flexibility of cultured cell lines7-10. In particular, mouse stem cell-derived neurons (ESNs) have been found to be highly sensitive to physiological doses of BoNT/A-/G and to replicate many in vivo responses to intoxication, including differential persistences, activity-enhanced intoxication, and serotype-specific potencies5,8,11. These behaviors suggest that in vivo mechanisms of BoNT uptake, processing, trafficking and activity are conserved in ESNs. However, inhibition of synaptic activity is the signature manifestation of botulism, and therefore demonstrating a loss of synaptic activity following intoxication by CNTs is essential before concluding that ESNs are a suitable in vitro derived cell-based model for CNT studies.
To measure the effects of intoxication with CNTs on synaptic activity, whole-cell patch-clamp electrophysiology was used to quantify monosynaptic currents in vehicle-treated or CNT-treated DIV 21+ ESNs. We found that intoxication of ESNs with BoNT/A-/G or TeNT caused &#62;95% loss of synaptic activity within 20 hr in all cases. Further characterization conducted 20 hr after intoxication with BoNT/A revealed a dose-dependent effect on synaptic activity, with a limit of detection below 0.005 pM and an IC50 value of 0.013 pM. These findings indicate that the sensitivity and time frame of electrophysiological detection of intoxication are considerably improved over comparable immunoblot-based analyses of SNAP-25 cleavage and in vivo mouse lethality assays, demonstrating that functional measurements of intoxication in synaptically active neuron cultures may facilitate more sensitive, specific and rapid methods to characterize the cellular response to BoNT.

<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>Table 1. ESC and ESN</td>
		</tr>
		<tr>
			<td>Knockout DMEM</td>
			<td>Life Technologies</td>
			<td>10829-018</td>
			<td>Media: ESC culture medium 
			Formulation and notes: 500 mL</td>
		</tr>
		<tr>
			<td>100x MEM NEAA</td>
			<td>Life Technologies</td>
			<td>11140-050</td>
			<td>Media: store at 4 &#176;C for up to 1 month 
			Formulation and notes: 6 mL</td>
		</tr>
		<tr>
			<td>200 mM L-Alanyl-L-Glutamine</td>
			<td>ATCC</td>
			<td>30-2115</td>
			<td>6 mL</td>
		</tr>
		<tr>
			<td>ES qualified FBS</td>
			<td>Applied Stem Cell</td>
			<td>ASM-5007</td>
			<td>90 mL</td>
		</tr>
		<tr>
			<td>100x antibiotics</td>
			<td>Sigma-Aldrich</td>
			<td>A5955</td>
			<td>3 mL</td>
		</tr>
		<tr>
			<td>55 mM 2-mercaptoethanol</td>
			<td>Life Technologies</td>
			<td>21985-023</td>
			<td>1.1 mL</td>
		</tr>
		<tr>
			<td>107 Units/mL LIF</td>
			<td>Millipore</td>
			<td>ESG1107</td>
			<td>60 &#956;L</td>
		</tr>
		<tr>
			<td>Knockout DMEM</td>
			<td>Life Technologies</td>
			<td>10829-018</td>
			<td>Media: ESC differentiation medium 
			Formulation and notes: 436.6 mL</td>
		</tr>
		<tr>
			<td>100x MEM NEAA</td>
			<td>Life Technologies</td>
			<td>11140-050</td>
			<td>Media: store at 4 &#176;C for up to 1 month 
			Formulation and notes: 5 mL</td>
		</tr>
		<tr>
			<td>200 mM L-Alanyl-L-Glutamine</td>
			<td>ATCC</td>
			<td>30-2115</td>
			<td>5 mL</td>
		</tr>
		<tr>
			<td>ESC-qualified serum</td>
			<td>Applied Stem Cell</td>
			<td>ASM-5007</td>
			<td>50 mL</td>
		</tr>
		<tr>
			<td>100x antibiotics</td>
			<td>Sigma-Aldrich</td>
			<td>A5955</td>
			<td>2.5 mL</td>
		</tr>
		<tr>
			<td>55 mM 2-mercaptoethanol</td>
			<td>Life Technologies</td>
			<td>21985-023</td>
			<td>0.9 mL</td>
		</tr>
		<tr>
			<td>Dulbecco&#39;s PBS</td>
			<td>Sigma-Aldrich</td>
			<td>D8537</td>
			<td>Media: NPC trypsinization medium 
			Formulation and notes: 100 mL</td>
		</tr>
		<tr>
			<td>0.5 M EDTA (18.3%)</td>
			<td>Sigma-Aldrich</td>
			<td>3690</td>
			<td>Media: freeze in 5 mL aliquote 
			Formulation and notes: 0.266 mL</td>
		</tr>
		<tr>
			<td>Trypsin</td>
			<td>Sigma-Aldrich</td>
			<td>T8802</td>
			<td>50 mg</td>
		</tr>
		<tr>
			<td>Polyethyleneimine (PEI)</td>
			<td>Sigma-Aldrich</td>
			<td>P3143</td>
			<td>Media: Surface coating solutions 
			Formulation and notes: 2.5 &#181;g/mL in H20</td>
		</tr>
		<tr>
			<td>Poly-D-lysine (PDL)</td>
			<td>Sigma-Aldrich</td>
			<td>P7280</td>
			<td>Media: use within 1 wk 
			Formulation and notes: 100 &#181;g/mL in H20</td>
		</tr>
		<tr>
			<td>Laminin</td>
			<td>Sigma-Aldrich</td>
			<td>L2020</td>
			<td>5 &#181;g/mL in H20</td>
		</tr>
		<tr>
			<td>DMEM/F12 + GlutaMAX</td>
			<td>Life Technologies</td>
			<td>10565-018</td>
			<td>Media: NPC culture medium 
			Formulation and notes: 492.5 mL</td>
		</tr>
		<tr>
			<td>100x N2 vitamins</td>
			<td>Life Technologies</td>
			<td>17502-048</td>
			<td>Media: store at 4 &#176;C for up to 1 month 
			Formulation and notes: 5 mL</td>
		</tr>
		<tr>
			<td>100x antibiotics</td>
			<td>Sigma-Aldrich</td>
			<td>A5955</td>
			<td>2.5 mL</td>
		</tr>
		<tr>
			<td>Neurobasal A</td>
			<td>Life Technologies</td>
			<td>10888-022</td>
			<td>Media: ESN culture medium 
			Formulation and notes: 482.5 mL</td>
		</tr>
		<tr>
			<td>50x B27 vitamins</td>
			<td>Life Technologies</td>
			<td>17504-044</td>
			<td>Media: store at 4 &#176;C for up 1 month 
			Formulation and notes: 10 mL</td>
		</tr>
		<tr>
			<td>200 mM L-Alanyl-L-Glutamine</td>
			<td>ATCC</td>
			<td>30-2115</td>
			<td>5 mL</td>
		</tr>
		<tr>
			<td>100x antibiotics</td>
			<td>Sigma-Aldrich</td>
			<td>A5955</td>
			<td>2.5 mL</td>
		</tr>
		<tr>
			<td>5-fluoro-2&#39;-deoxyuridine (5FDU)</td>
			<td>Sigma-Aldrich</td>
			<td>F0503</td>
			<td>Media: 2000x Mitotic inhibitors aliquot and store at -20 &#176;C 
			Formulation and notes: dd 150 mg 5FDU and 350 mg uridine to 10 mL Neurobasal A. Sterile filter, aliquot and freeze. Use 2000x in ESN culture medium.</td>
		</tr>
		<tr>
			<td>Uridine</td>
			<td>Sigma-Aldrich</td>
			<td>U3003</td>
			<td></td>
		</tr>
		<tr>
			<td>TrypLE Express Trypsin</td>
			<td>Life Technologies</td>
			<td>12605-010</td>
			<td>Media: Miscellaneous 
			Formulation and notes: store at RT</td>
		</tr>
		<tr>
			<td>DMSO</td>
			<td>Sigma-Aldrich</td>
			<td>D8418</td>
			<td>store at RT</td>
		</tr>
		<tr>
			<td>soybean trypsin inhibitor (STI)</td>
			<td>Sigma-Aldrich</td>
			<td>T6414</td>
			<td>store at -20 &#176;C</td>
		</tr>
		<tr>
			<td>ethanol</td>
			<td>Sigma-Aldrich</td>
			<td>E7023</td>
			<td>store at RT</td>
		</tr>
		<tr>
			<td>ascorbic acid</td>
			<td>Sigma-Aldrich</td>
			<td>A4403</td>
			<td>Prepare 100 mM stock by dissolving 100 mg ascorbic acid in 5.7 mL of 50:50 DMSO/ethanol mix.</td>
		</tr>
		<tr>
			<td>retinoic acid (RA)</td>
			<td>Sigma-Aldrich</td>
			<td>R2625</td>
			<td>Resuspend 15 mg RA in 9 mL 50:50 DMSO/ethanol. Supplement with 1 mL of 100 mM ascorbic acid stock. Aliquot and stored at -80 &#176;C. Stable for 6 mos.</td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>Table 2. MIST</td>
		</tr>
		<tr>
			<td>NaCl</td>
			<td>Sigma-Aldrich</td>
			<td>71386</td>
			<td>Media: Extracellular Recording Buffer 
			Final Concentration (mM): 58.44 
			MW: 140</td>
		</tr>
		<tr>
			<td>KCl</td>
			<td>Sigma-Aldrich</td>
			<td>60135</td>
			<td>Media: (ERB; pH = 7.3, 315 mO) 
			Final Concentration (mM): 74.56 
			MW: 3.5</td>
		</tr>
		<tr>
			<td>NaH2PO4</td>
			<td>Sigma-Aldrich</td>
			<td>S3139</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 119.98 
			MW: 1.25</td>
		</tr>
		<tr>
			<td>CaCl2</td>
			<td>Sigma-Aldrich</td>
			<td>21115</td>
			<td>Final Concentration (mM): 110.98 
			MW: 2</td>
		</tr>
		<tr>
			<td>MgCl2</td>
			<td>Sigma-Aldrich</td>
			<td>63069</td>
			<td>Final Concentration (mM): 95.21 
			MW: 1</td>
		</tr>
		<tr>
			<td>D-glucose</td>
			<td>Sigma-Aldrich</td>
			<td>G8644</td>
			<td>Final Concentration (mM): 180.16 
			MW: 10</td>
		</tr>
		<tr>
			<td>HEPES</td>
			<td>Sigma-Aldrich</td>
			<td>H0887</td>
			<td>Final Concentration (mM): 238.3 
			MW: 10</td>
		</tr>
		<tr>
			<td>K-gluconate</td>
			<td>Sigma-Aldrich</td>
			<td>P1847</td>
			<td>Media: Intracellular Recording Buffer 
			Final Concentration (mM): 234.5 
			MW: 140</td>
		</tr>
		<tr>
			<td>NaCl</td>
			<td>Sigma-Aldrich</td>
			<td>71386</td>
			<td>Media: (IRB; pH = 7.3, 320 mO) 
			Final Concentration (mM): 58.44 
			MW: 5</td>
		</tr>
		<tr>
			<td>Mg-ATP</td>
			<td>Sigma-Aldrich</td>
			<td>A9187</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 507.18 
			MW: 2</td>
		</tr>
		<tr>
			<td>Li-GTP</td>
			<td>Sigma-Aldrich</td>
			<td>G5884</td>
			<td>Final Concentration (mM): 523.18 
			MW: 0.5</td>
		</tr>
		<tr>
			<td>CaCl2</td>
			<td>Sigma-Aldrich</td>
			<td>21115</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 110.98 
			MW: 0.1</td>
		</tr>
		<tr>
			<td>MgCl2</td>
			<td>Sigma-Aldrich</td>
			<td>63069</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 95.21 
			MW: 1</td>
		</tr>
		<tr>
			<td>EGTA</td>
			<td>Sigma-Aldrich</td>
			<td>E3889</td>
			<td>380.35</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 380.35 
			MW: 1</td>
		</tr>
		<tr>
			<td>HEPES</td>
			<td>Sigma-Aldrich</td>
			<td>H0887</td>
			<td>Media: Stable at 4 &#176;C for at least 6 mo. 
			Final Concentration (mM): 238.3 
			MW: 10</td>
		</tr>
		<tr>
			<td>bicuculline</td>
			<td>Tocris</td>
			<td>131</td>
			<td>Media: Miscellaneous 
			Final Concentration (mM): 0.01 
			MW: 417.85</td>
		</tr>
		<tr>
			<td>CNQX</td>
			<td>Sigma-Aldrich</td>
			<td>C239</td>
			<td>Final Concentration (mM): 0.01 
			MW: 276.12</td>
		</tr>
		<tr>
			<td>Tetrodotoxin</td>
			<td>Sigma-Aldrich</td>
			<td>A8001</td>
			<td>Final Concentration (mM): 0.005 
			MW: 645.74</td>
		</tr>
		<tr>
			<td>BoNT/A-/G</td>
			<td>Metabiologics</td>
			<td>N/A</td>
			<td>Media: 
			Final Concentration (mM): TBD 
			MW: 150,000</td>
		</tr>
		<tr>
			<td>Tetanus toxin</td>
			<td>Sigma-Aldrich</td>
			<td>T3194</td>
			<td>Final Concentration (mM): TBD 
			MW: 150,000</td>
		</tr>
		<tr>
			<td>Sigmacote</td>
			<td>Sigma-Aldrich</td>
			<td>SL-2</td>
			<td>Final Concentration (mM): N/A 
			MW: N/A</td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>Table 3. Equipment and Software</td>
		</tr>
		<tr>
			<td>MiniAnalysis (version 6.0.7)</td>
			<td>Synaptosoft, Inc.</td>
			<td>N/A</td>
			<td>Event detection software</td>
		</tr>
		<tr>
			<td>Igor Pro (version 6.22A)</td>
			<td>WaveMetrics</td>
			<td>N/A</td>
			<td>Software for visualization of recordings</td>
		</tr>
		<tr>
			<td>Patchmaster</td>
			<td>Heka</td>
			<td>N/A</td>
			<td>Data acquisition software</td>
		</tr>
		<tr>
			<td>Olympus IX51 inverted microscope</td>
			<td>Olympus</td>
			<td>N/A</td>
			<td></td>
		</tr>
		<tr>
			<td>micromanipulator</td>
			<td>Sutter Instrument</td>
			<td>MPC-365</td>
			<td></td>
		</tr>
		<tr>
			<td>patch-clamp amplifier</td>
			<td>Heka</td>
			<td>ECB10USB</td>
			<td></td>
		</tr>
		<tr>
			<td>micropipette puller</td>
			<td>Sutter Instrument</td>
			<td>P-1000</td>
			<td></td>
		</tr>
		<tr>
			<td>borosilicate capillary tubes</td>
			<td>Sutter Instrument</td>
			<td>B150-86-10</td>
			<td>Corning 7740</td>
		</tr>
		<tr>
			<td>18 mm glass coverslips</td>
			<td>Fisher</td>
			<td>12-545-84</td>
			<td></td>
		</tr>
		<tr>
			<td>plasma cleaner</td>
			<td>Harrick Plasma</td>
			<td>PDC-32G</td>
			<td></td>
		</tr>
		<tr>
			<td>cell strainer (40 &#181;m)</td>
			<td>Fisher</td>
			<td>08-771-1</td>
			<td></td>
		</tr>
		<tr>
			<td>Stovall Belly Dancer Shaker</td>
			<td>Fisher</td>
			<td>15-453-211</td>
			<td></td>
		</tr>
		<tr>
			<td>low adhesion dishes</td>
			<td>Fisher</td>
			<td>05-539-101</td>
			<td>Corning 3262</td>
		</tr>
		<tr>
			<td>bacterial dishes</td>
			<td>VWR</td>
			<td>25384-302</td>
			<td>100 x 15 mm</td>
		</tr>
	</tbody>
</table>

functional evaluation of biological neurotoxins in networked cultures of stem cell-derived central nervous system neurons

Therapeutic and mechanistic studies of the presynaptically targeted clostridial neurotoxins (CNTs) have been limited by the need for a scalable, cell-based model that produces functioning synapses and undergoes physiological responses to intoxication. Here we describe a simple and robust method to efficiently differentiate murine embryonic stem cells (ESCs) into defined lineages of synaptically active, networked neurons. Following an 8 day differentiation protocol, mouse embryonic stem cell-derived neurons (ESNs) rapidly express and compartmentalize neurotypic proteins, form neuronal morphologies and develop intrinsic electrical responses. By 18 days after differentiation (DIV 18), ESNs exhibit active glutamatergic and &#947;-aminobutyric acid (GABA)ergic synapses and emergent network behaviors characterized by an excitatory:inhibitory balance. To determine whether intoxication with CNTs functionally antagonizes synaptic neurotransmission, thereby replicating the in vivo pathophysiology that is responsible for clinical manifestations of botulism or tetanus, whole-cell patch clamp electrophysiology was used to quantify spontaneous miniature excitatory post-synaptic currents (mEPSCs) in ESNs exposed to tetanus neurotoxin (TeNT) or botulinum neurotoxin (BoNT) serotypes /A-/G. In all cases, ESNs exhibited near-complete loss of synaptic activity within 20 hr. Intoxicated neurons remained viable, as demonstrated by unchanged resting membrane potentials and intrinsic electrical responses. To further characterize the sensitivity of this approach, dose-dependent effects of intoxication on synaptic activity were measured 20 hr after addition of BoNT/A. Intoxication with 0.005 pM BoNT/A resulted in a significant decrement in mEPSCs, with a median inhibitory concentration (IC50) of 0.013 pM. Comparisons of median doses indicate that functional measurements of synaptic inhibition are faster, more specific and more sensitive than SNARE cleavage assays or the mouse lethality assay. These data validate the use of synaptically coupled, stem cell-derived neurons for the highly specific and sensitive detection of CNTs.

We have developed a differentiation protocol that enables the economic production of large quantities of highly pure stem cell-derived neurons from mouse ESCs (detailed in Figure 1A)8,11. This method has been used over a period of years to reproducibly differentiate privately generated and commercially available ESC lines into neurons of defined lineages12-14. Critical elements of this protocol include (1) adaptation of ESCs to feeder cell-free suspension culture; (2) proper maintenance of suspension cultures; and (3) differentiation under rotary conditions. Transition to suspension culture dramatically reduces the time and cost of ESC maintenance, and obviates the need to remove feeder cells prior to differentiation. Following suspension adaptation, Oct3/4 expression is consistent through at least 30 passages, indicating that suspension adaptation does not alter expression of pluripotency markers (Figure 1B-D). ESCs are suitable for neuronal differentiation once cell yield consistently exceeds 1 x 107 cells per passage. This typically occurs within ten passages after suspension adaptation or five passages after thawing of ESCs that were previously suspension-adapted. Mechanical rotation of differentiating aggregates was also found to be critical to increased neuronal yield. The addition of a rotary shaker eliminated super-aggregate formation, increasing aggregate viability and producing a ~300% increase in the yield of neural progenitor cells (NPCs) at DIV 0 (Figure 1E).
A typical differentiation starts with 3.5 x 106 ESCs at DIV -8 and produces 115 x 106 NPCs at DIV 0, roughly 60% of which will survive and become neurons. The remaining 40% comprise non-neuronal cells and are largely eliminated by serum deprivation between DIV 0 - 1. The small number of persisting glia can be removed by addition of mitotic inhibitors from DIV 2 - 4 or DIV 8 - 12. Plating density is critical at DIV 0; neurons plated too sparsely will not survive beyond 2 weeks. Within days of plating, differentiated neurons exhibit neuronal morphologies and compartmentalize neurotypic proteins, such as the somatodendritic marker MAP2 and the axonal marker Tau (Figure 2A). By DIV 14 synapsin-1+ puncta can be identified at axodendritic interfaces, suggestive of synapse formation. This is consistent with the expression of synaptic marker proteins prior to DIV 7 8,11. Neuronal morphologies continue to mature through DIV 21, at which time cultures exhibit elaborate axodendritic arbors and large synaptic puncta (Figure 2A). If maintained appropriately, ESNs remain viable and active for at least 4 weeks after plating.
Longitudinal expression profiling using RNA-sequencing corroborated morphological and proteomic evidence of neuronal specification and maturation11,15. Representative markers of developmental progression exhibited stage-specific expression profiles, including Oct3/4, Nestin, DCX, NeuN and KCC2 (Figure 2B). By DIV 0, ESNs expressed abundant copies of neuron-specific structural proteins, including MAP2 and Tau. Consistent with previous findings, markers for only two neuronal subtypes were observed: vGluT2-expressing midbrain/hindbrain glutamatergic neurons and GABAergic interneurons8. Correspondingly, a wide array of glutamatergic and GABAergic markers exhibited sharp increases in expression between DIV 0 and DIV 7, including pre-synaptic SNARE proteins required for neurotransmitter release; neurotransmitter receptors required for post-synaptic responses; and scaffolding proteins required to tether these receptors to the post-synaptic membrane. Neurons exhibit mature intrinsic electrical characteristics by DIV 14 and spontaneous miniature excitatory post-synaptic currents by DIV 16 16.
The Measured Inhibition of Synaptic Transmission (MIST) assay was used to evaluate the effect of intoxication on synaptic activity. By comparing mEPSC frequencies between intoxicated and vehicle-treated DIV 24+ ESNs, MIST provides a quantitative and specific measurement of intoxication based on the functional inhibition of synaptic activity (Figure 3A). MIST was used to measure the effects of BoNT/A-/G or TeNT on synaptic activity in ESNs at 20 hr after bath addition of each toxin. Toxins were added at a concentration equivalent to 10-fold the EC50 value, as previously determined by immunoblot analysis of SNARE protein cleavage11. All toxins reduced mEPSC frequencies to less than 5% of vehicle-treated controls. Reductions in synaptic rates were not attributable to cell death or altered intrinsic responses, since intoxicated ESNs were capable of being patched, fired repeated action potentials in response to current injection and exhibited no significant alteration in resting membrane potential (Figure 3B,C).
To compare the sensitivity of MIST to existing methods to detect CNTs, the limit of detection and median inhibitory concentration (IC50) were determined 20 hr after addition of BoNT/A to ESNs. Intoxication by as little as 0.005 pM BoNT/A produced a statistically significant reduction in mEPSC frequency, with an IC50 value of 0.013 pM and complete silencing of synaptic activity above 0.5 pM (Figure 4A). This IC50 value corresponds to approximately 0.5 mouse lethal units/ml, suggesting that MIST is twice as sensitive and 2- to 4-fold faster than the MLA in detecting the presence of BoNT/A. Immunoblot measurements of SNAP-25 cleavage produced an EC50 value of 0.38 pM and a minimum detectable dose of 0.05 pM, indicating that MIST is approximately 30-fold more sensitive than immunoblot-based detection of cleaved SNARE proteins (Figure 4B).
<img alt="Figure 1" src="/files/ftp_upload/52361/52361fig1.jpg" /> 
Figure 1. Suspension-adapted ESNs remain mitotically stable and express markers of pluripotency. (A) Schematic of ESC maintenance and differentiation. The presence or absence of retinoic acid (RA) or leukemia inhibitory factor (LIF) is marked by a + or &#8211;. A comparison between days in vitro (DIV) and classical developmental stages (DS) for primary neuron cultures is provided17. (B) Proliferation rates for R1, D3 and C57BL/6J ES cell lines stabilize by five passages after transition to suspension culture. (C) Flow cytometry data demonstrate no substantive change in Oct3/4 expression in the R1, D3 and C57BL/6J ES cell lines measured over 25 passages in suspension culture (n = 6 for each). (D) Actual cell yields during routine passaging for a suspension-adapted R1 ESC line measured between passages 5 and 30 (black line). Theoretical cumulative yields if no cells are discarded during passaging are also presented (red line). (E) Bright-field images of DIV 0 aggregates produced under static (left) or rotary conditions (right). Rotary conditions produced spherical aggregates without agglomeration and increased NPC yields 3-fold (p &#60; 0.001, determined using Student&#8217;s t-test)11. * indicates a P &#60; 0.05. This figure has been modified from Hubbard et al.11 <a href="https://www.jove.com/files/ftp_upload/52361/52361fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" src="/files/ftp_upload/52361/52361fig2.jpg" /> 
Figure 2. Morphological, proteomic and transcriptomic evidence of neuronal specification and maturation. (A) Immunocytochemistry from DIV 7 &#8211; DIV 49 demonstrates neuronal arborization and the appearance of synaptic puncta at axodendritic interfaces. Axons are labeled with Tau (green), dendrites are labeled with MAP2 (red), pre-synaptic compartments are labeled with synapsin (white), and nuclei are stained with DAPI (blue). (B) Longitudinal expression profiling of representative genes demonstrating developmental stage-specific expression and specifying neuronal subtypes. All gene transcripts are expressed as approximate number of transcripts per cell. <a href="https://www.jove.com/files/ftp_upload/52361/52361fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/52361/52361fig3.jpg" /> 
Figure 3. ESNs undergo inhibition of synaptic activity when exposed to BoNT/A-G and TeNT. (A) Representative traces from ESNs collected 20 hr after bath addition of ~10 x EC50 values of BoNT/A - /G, TeNT or vehicle. Each neurotoxin reduced synaptic activity by over 95% in comparison to controls. (B) Intoxicated neurons remained able to fire repeated APs in response to depolarizing current injection (as demonstrated for BoNT/A, but observed in all intoxicated cultures) and (C) exhibited no changes in the negative resting membrane potential (C; n &#62; 18 for each treatment). <a href="https://www.jove.com/files/ftp_upload/52361/52361fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" src="/files/ftp_upload/52361/52361fig4.jpg" /> 
Figure 4. Determination of the sensitivity of MIST in BoNT/A-treated ESNs. (A) MIST measurements of synaptic activity 20 hr after bath addition of BoNT/A. Representative voltage-clamp trace segments exhibited a decrease in mEPSC frequency following BoNT/A exposure (left side). Quantitation of mEPSC frequency (bar graph, right side, n = 20 for controls; n = 11 - 22 for each dose) confirms a dose-dependent decrease in mEPSC frequency. The median inhibitory concentration was determined with a least-squares fit of a non-linear regression using a four parameter variable slope (R2 &#62; 0.91). Note the limit of detection by MIST in ESNs is at least 0.005 pM. (B) BoNT/A intoxication of ESNs results in cleavage of SNAP-25 as visualized by gel mobility shifts (a representative western blot on the left side with a bar graph showing quantification of SNAP-25 cleavage on the right; n = 4). Note the decreased sensitivity using SNARE protein cleavage (SNAP-25) as an endpoint (EC50 of 0.36 pM) vs. MIST (IC50 of 0.013 pM). * indicates a P &#60; 0.05; *** indicates a P &#60; 0.001. <a href="https://www.jove.com/files/ftp_upload/52361/52361fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Functional Evaluation of Biological Neurotoxins in Networked Cultures of Stem Cell-derived Central Nervous System Neurons at JoVE.com

Functional Evaluation of Biological Neurotoxins in Networked Cultures of Stem Cell-derived Central Nervous System Neurons

A custom protocol is described to differentiate mouse ES cells into defined populations of highly pure neurons exhibiting functioning synapses and emergent network behavior. Electrophysiological analysis demonstrates the loss of synaptic transmission following exposure to botulinum neurotoxin serotypes /A-/G and tetanus neurotoxin.

Therapeutic and mechanistic studies of the presynaptically targeted clostridial neurotoxins (CNTs) have been limited by the need for a scalable, ...

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9.3K vues.  United States Army Medical Research Institute of Chemical Defense. A custom protocol is described to differentiate mouse ES cells into defined populations of highly pure neurons exhibiting functioning synapses and emergent network behavior. Electrophysiological analysis demonstrates the loss of synaptic transmission following exposure to botulinum neurotoxin serotypes /A-/G and tetanus neurotoxin.

Vidéo: Functional Evaluation of Biological Neurotoxins in Networked Cultures of Stem Cell-derived Central Nervous System Neurons

Multimodal Imaging of Stem Cell Implantation in the Central Nervous System of Mice

During the past decade, stem cell transplantation has gained increasing interest as primary or secondary therapeutic modality for a variety of diseases, both in preclinical and clinical studies. However, to date results regarding functional outcome and/or tissue regeneration following stem cell transplantation are quite diverse. Generally, a clinical benefit is observed without profound understanding of the underlying mechanism(s)1. Therefore, multiple efforts have led to the development of different molecular imaging modalities to monitor stem cell grafting with the ultimate aim to accurately evaluate survival, fate and physiology of grafted stem cells and/or their micro-environment. Changes observed in one or more parameters determined by molecular imaging might be related to the observed clinical effect. In this context, our studies focus on the combined use of bioluminescence imaging (BLI), magnetic resonance imaging (MRI) and histological analysis to evaluate stem cell grafting.
BLI is commonly used to non-invasively perform cell tracking and monitor cell survival in time following transplantation2-7, based on a biochemical reaction where cells expressing the Luciferase-reporter gene are able to emit light following interaction with its substrate (e.g. D-luciferin)8, 9. MRI on the other hand is a non-invasive technique which is clinically applicable10 and can be used to precisely locate cellular grafts with very high resolution11-15, although its sensitivity highly depends on the contrast generated after cell labeling with an MRI contrast agent. Finally, post-mortem histological analysis is the method of choice to validate research results obtained with non-invasive techniques with highest resolution and sensitivity. Moreover end-point histological analysis allows us to perform detailed phenotypic analysis of grafted cells and/or the surrounding tissue, based on the use of fluorescent reporter proteins and/or direct cell labeling with specific antibodies.
In summary, we here visually demonstrate the complementarities of BLI, MRI and histology to unravel different stem cell- and/or environment-associated characteristics following stem cell grafting in the CNS of mice. As an example, bone marrow-derived stromal cells, genetically engineered to express the enhanced Green Fluorescent Protein (eGFP) and firefly Luciferase (fLuc), and labeled with blue fluorescent micron-sized iron oxide particles (MPIOs), will be grafted in the CNS of immune-competent mice and outcome will be monitored by BLI, MRI and histology (Figure 1).

This article describes an optimized sequence of events for multimodal imaging of cellular grafts in rodent brain using: (i) in vivo bioluminescence and magnetic resonance imaging, and (ii) post mortem histological analysis. Combining these imaging modalities on a single animal allows cellular graft evaluation with high resolution, sensitivity and specificity.

During the past decade, stem cell transplantation has gained increasing interest as primary or secondary therapeutic modality for a variety of diseases, ...

Production of Lentiviral Vectors for Transducing Cells from the Central Nervous System

Efficient gene delivery in the central nervous system (CNS) is important in studying gene functions, modeling neurological diseases and developing therapeutic approaches. Lentiviral vectors are attractive tools in transduction of neurons and other cell types in CNS as they transduce both dividing and non-dividing cells, support sustained expression of transgenes, and have relatively large packaging capacity and low toxicity 1-3. Lentiviral vectors have been successfully used in transducing many neural cell types in vitro 4-6 and in animals 7-10.
Great efforts have been made to develop lentiviral vectors with improved biosafety and efficiency for gene delivery. The current third generation replication-defective and self-inactivating (SIN) lentiviral vectors are depicted in Figure 1. The required elements for vector packaging are split into four plasmids. In the lentiviral transfer plasmid, the U3 region in the 5' long terminal repeat (LTR) is replaced with a strong promoter from another virus. This modification allows the transcription of the vector sequence independent of HIV-1 Tat protein that is normally required for HIV gene expression 11. The packaging signal (&Psi;) is essential for encapsidation and the Rev-responsive element (RRE) is required for producing high titer vectors. The central polypurine tract (cPPT) is important for nuclear import of the vector DNA, a feature required for transducing non-dividing cells 12. In the 3' LTR, the cis-regulatory sequences are completely removed from the U3 region. This deletion is copied to 5' LTR after reverse transcription, resulting in transcriptional inactivation of both LTRs. Plasmid pMDLg/pRRE contains HIV-1 gag/pol genes, which provide structural proteins and reverse transcriptase. pRSV-Rev encodes Rev which binds to the RRE for efficient RNA export from the nucleus. pCMV-G encodes the vesicular stomatitis virus glycoprotein (VSV-G) that replaces HIV-1 Env. VSV-G expands the tropism of the vectors and allows concentration via ultracentrifugation 13. All the genes encoding the accessory proteins, including Vif, Vpr, Vpu, and Nef are excluded in the packaging system. The production and manipulation of lentiviral vectors should be carried out according to NIH guidelines for research involving recombinant DNA (<a href="http://oba.od.nih.gov/oba/rac/Guidelines/NIH_Guidelines.pdf" target="_blank">http://oba.od.nih.gov/oba/rac/Guidelines/NIH_Guidelines.pdf</a>). An approval from individual Institutional Biological and Chemical Safety Committee may be required before using lentiviral vectors. Lentiviral vectors are commonly produced by cotransfection of 293T cells with lentiviral transfer plasmid and the helper plasmids encoding the proteins required for vector packaging. Many lentiviral transfer plasmids and helper plasmids can be obtained from Addgene, a non-profit plasmid repository (<a href="http://www.addgene.org/" target="_blank">http://www.addgene.org/</a>). Some stable packaging cell lines have been developed, but these systems provide less flexibility and their packaging efficiency generally declines over time 14, 15. Commercially available transfection kits may support high efficiency of transfection 16, but they can be very expensive for large scale vector preparations. Calcium phosphate precipitation methods provide highly efficient transfection of 293T cells and thus provide a reliable and cost effective approach for lentiviral vector production.
In this protocol, we produce lentiviral vectors by cotransfection of 293T cells with four plasmids based on the calcium phosphate precipitation principle, followed by purification and concentration with ultracentrifugation through a 20% sucrose cushion. The vector titers are determined by fluorescence- activated cell sorting (FACS) analysis or by real time qPCR. The production and titration of lentiviral vectors in this protocol can be finished with 9 days. We provide an example of transducing these vectors into murine neocortical cultures containing both neurons and astrocytes. We demonstrate that lentiviral vectors support high efficiency of transduction and cell type-specific gene expression in primary cultured cells from CNS.

In this protocol we describe production, purification and titration of lentiviral vectors. We provide an example of lentiviral vector-mediated gene delivery in primary cultured neurons and astrocytes. Our methods may also apply to other cell types in vitro and in vivo.

Efficient gene delivery in the central nervous system (CNS) is important in studying gene functions, modeling neurological diseases and developing ...

Labeling of Single Cells in the Central Nervous System of Drosophila melanogaster

In this article we describe how to individually label neurons in the embryonic CNS of Drosophila melanogaster by juxtacellular injection of the lipophilic fluorescent membrane marker DiI. This method allows the visualization of neuronal cell morphology in great detail. It is possible to label any cell in the CNS: cell bodies of target neurons are visualized under DIC optics or by expression of a fluorescent genetic marker such as GFP. After labeling, the DiI can be transformed into a permanent brown stain by photoconversion to allow visualization of cell morphology with transmitted light and DIC optics. Alternatively, the DiI-labeled cells can be observed directly with confocal microscopy, enabling genetically introduced fluorescent reporter proteins to be colocalised. The technique can be used in any animal, irrespective of genotype, making it possible to analyze mutant phenotypes at single cell resolution.

Labeling of Single Cells in the Central Nervous System of Drosophila melanogaster

We present a technique for labeling single neurons in the central nervous system (CNS) of Drosophila embryos, which allows the analysis of neuronal morphology by either transmitted light or confocal microscopy.

In this  article we describe how to individually label neurons in the embryonic CNS of Drosophila melanogaster by juxtacellular injection of the ...

An Injury Paradigm to Investigate Central Nervous System Repair in Drosophila

An experimental method has been developed to investigate the cellular responses to central nervous system (CNS) injury using the fruit-fly Drosophila. Understanding repair and regeneration in animals is a key question in biology. The damaged human CNS does not regenerate, and understanding how to promote the regeneration is one of main goals of medical neuroscience. The powerful genetic toolkit of Drosophila can be used to tackle the problem of CNS regeneration.
A lesion to the CNS ventral nerve cord (VNC, equivalent to the vertebrate spinal cord) is applied manually with a tungsten needle. The VNC can subsequently be filmed in time-lapse using laser scanning confocal microscopy for up to 24 hr to follow the development of the lesion over time. Alternatively, it can be cultured, then fixed and stained using immunofluorescence to visualize neuron and glial cells with confocal microscopy. Using appropriate markers, changes in cell morphology and cell state as a result of injury can be visualized. With ImageJ and purposely developed plug-ins, quantitative and statistical analyses can be carried out to measure changes in wound size over time and the effects of injury in cell proliferation and cell death. These methods allow the analysis of large sample sizes. They can be combined with the powerful genetics of Drosophila to investigate the molecular mechanisms underlying CNS regeneration and repair.

An Injury Paradigm to Investigate Central Nervous System Repair in Drosophila

An injury paradigm using the Drosophila larval ventral nerve cord to investigate central nervous system regeneration and repair is described. Stabbing followed by laser scanning confocal microscopy in time-lapse and fixed specimens, combined with quantitative analysis with purposefully developed software and genetics, are used to investigate the molecular mechanisms of CNS regeneration and repair.

An experimental method has been developed to investigate the cellular responses to central nervous system (CNS) injury using the fruit-fly Drosophila. ...

Direct Intraventricular Delivery of Drugs to the Rodent Central Nervous System

Due to an inability to cross the blood brain barrier, certain drugs need to be directly delivered into the central nervous system (CNS). Our lab focuses specifically on antisense oligonucleotides (ASOs), though the techniques shown in the video here can also be used to deliver a plethora of other drugs to the CNS. Antisense oligonucleotides (ASOs) have the capability to knockdown sequence-specific targets 1 as well as shift isoform ratios of specific genes 2. To achieve widespread gene knockdown or splicing in the CNS of mice, the ASOs can be delivered into the brain using two separate routes of administration, both of which we demonstrate in the video.
The first uses Alzet osmotic pumps, connected to a catheter that is surgically implanted into the lateral ventricle. This allows the ASOs to be continuously infused into the CNS for a designated period of time. The second involves a single bolus injection of a high concentration of ASO into the right lateral ventricle. Both methods use the mouse cerebral ventricular system to deliver the ASO to the entire brain and spinal cord, though depending on the needs of the study, one method may be preferred over the other.

We describe a method to target drugs to the central nervous system by either implanting a catheter or performing a bolus injection into the right lateral ventricle in mice. We focus specifically on the delivery of antisense oligonucleotides. This technique is readily adaptable to other drugs and to rats.

Due to an inability to cross the blood brain barrier, certain drugs need to be directly delivered into the central nervous system (CNS). Our lab focuses ...

In vivo Interrogation of Central Nervous System Translatome by Polyribosome Fractionation

Multiple processes are involved in gene expression including transcription, translation and stability of mRNAs and proteins. Each of these steps are tightly regulated, affecting the final dynamics of protein abundance. Various regulatory mechanisms exist at the translation step, rendering mRNA levels alone an unreliable indicator of gene expression. In addition, local regulation of mRNA translation has been particularly implicated in neuronal functions, shifting &#39;translatomics&#39; to the focus of attention in neurobiology. The presented method can be used to bridge transcriptomics and proteomics.
Here we describe essential modifications to the technique of polyribosome fractionation, which interrogates the translatome based on the association of actively translated mRNAs to multiple ribosomes and their differential sedimentation in sucrose gradients. Traditionally, working with in vivo samples, particularly of the central nervous system (CNS), has proven challenging due to the restricted amounts of material and the presence of fatty tissue components. In order to address this, the described protocol is specifically optimized for use with minimal amount of CNS material, as demonstrated by the use of single mouse spinal cord and brain. Briefly, CNS tissues are extracted and translating ribosomes are immobilized on mRNAs with cycloheximide. Myelin flotation is then performed to remove lipid rich components. Fractionation is performed on a sucrose gradient where mRNAs are separated according to their ribosomal loading. Isolated fractions are suitable for a range of downstream assays, including new genome wide assay technologies.

In vivo Interrogation of Central Nervous System Translatome by Polyribosome Fractionation

This protocol illustrates essential modifications of polyribosome fractionation in order to study the translatome of in vivo CNS samples. It allows global assessment of translation and transcription regulation through the isolation and comparison of total RNA to ribosome bound RNA fractions.

Multiple processes are involved in gene expression including transcription, translation and stability of mRNAs and proteins. Each of these steps are ...

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 ...

Optical Clearing of the Mouse Central Nervous System Using Passive CLARITY

Traditionally, tissue visualization has required that the tissue of interest be serially sectioned and imaged, subjecting each tissue section to unique non-linear deformations, dramatically hampering one's ability to evaluate cellular morphology, distribution and connectivity in the central nervous system (CNS). However, optical clearing techniques are changing the way tissues are visualized. These approaches permit one to probe deeply into intact organ preparations, providing tremendous insight into the structural organization of tissues in health and disease. Techniques such as Clear Lipid-exchanged Acrylamide-hybridized Rigid Imaging-compatible Tissue-hYdrogel (CLARITY) achieve this goal by providing a matrix that binds important biomolecules while permitting light-scattering lipids to freely diffuse out. Lipid removal, followed by refractive index matching, renders the tissue transparent and readily imaged in 3 dimensions (3D). Nevertheless, the electrophoretic tissue clearing (ETC) used in the original CLARITY protocol can be challenging to implement successfully and the use of a proprietary refraction index matching solution makes it expensive to use the technique routinely. This report demonstrates the implementation of a simple and inexpensive optical clearing protocol that combines passive CLARITY for improved tissue integrity and 2,2&#8242;-thiodiethanol (TDE), a previously described refractive index matching solution.

Optical clearing techniques are revolutionizing the way tissues are visualized. In this report we describe modifications of the original Clear Lipid-exchanged Acrylamide-hybridized Rigid Imaging-compatible Tissue-hYdrogel (CLARITY) protocol that yields more consistent and less expensive results.

Traditionally, tissue visualization has required that the tissue of interest be serially sectioned and imaged, subjecting each tissue section to unique ...

Methods and Tips for Intravenous Administration of Adeno-associated Virus to Rats and Evaluation of Central Nervous System Transduction

Adeno-associated virus (AAV) vectors are a key reagent in the neurosciences for clustered regularly interspaced short palindromic repeats (CRISPR), optogenetics, cre-lox targeting, etc. The purpose of this manuscript is to aid the investigator attempting expansive central nervous system (CNS) gene transfer in the rat via tail vein injection of AAV. Wide-scale expression is relevant for conditions with widespread pathology, and a rat model is significant due to its greater size and physiologic similarities to humans compared to mice. In this example application, a wide-scale neuronal transduction is used to mimic a neurodegenerative disease that affects the entire spinal cord, amyotrophic lateral sclerosis (ALS). The efficient wide-scale CNS transduction can also be used to deliver therapeutic protein factors in pre-clinical studies. After a post-injection expression interval of several weeks, the effects of the transduction are evaluated. For a green fluorescent protein (GFP) control vector, the amount of GFP in the cerebellum is estimated quickly and reliably by a basic imaging program. For motor disease phenotypes that are induced by the ALS related protein transactive response DNA-binding protein of 43 kDa (TDP-43), the deficits are scored by escape reflex and rotarod. Beyond disease modeling and gene therapy, there are diverse potential applications for the wide-scale gene targeting described here. The expanded use of this method will aid in expediting hypothesis testing in the neurosciences and neurogenetics.

Methods for a wide-scale central nervous system gene delivery in the rat are covered. In this example, the purpose is to mimic a disease that affects the entire spinal cord. The widespread transduction can be used to deliver a therapeutic protein to the CNS from a one-time, peripheral administration.

Adeno-associated virus (AAV) vectors are a key reagent in the neurosciences for clustered regularly interspaced short palindromic repeats (CRISPR), ...

Intrathecal Delivery of Antisense Oligonucleotides in the Rat Central Nervous System

The blood brain barrier (BBB) is an important defense against the entrance of potentially toxic or pathogenic agents from the blood into the central nervous system (CNS). However, its existence also dramatically lowers the accessibility of systemically administered therapeutic agents to the CNS. One method to overcome this, is to inject those agents directly into the cerebrospinal fluid (CSF), thus bypassing the BBB. This can be done via implantation of a catheter for either continuous infusion using an osmotic pump, or for single bolus delivery. In this article, we describe a surgical protocol for delivery of CNS-targeting antisense oligonucleotides (ASOs) via a catheter implanted directly into the cauda equina space of the adult rat spine. As representative results, we show the efficacy of a single bolus ASO intrathecal (IT) injection via this catheterization system in knocking down the target RNA in different regions of the rat CNS. The procedure is safe, effective and does not require expensive equipment or surgical tools. The technique described here can be adapted to deliver drugs in other modalities as well.

Here, we describe a method for delivering drugs to the rat central nervous system by implanting a catheter into the lumbar intrathecal space of the spine. We focus on the delivery of antisense oligonucleotides, though this method is suitable for delivery of other therapeutic modalities as well.

The blood brain barrier (BBB) is an important defense against the entrance of potentially toxic or pathogenic agents from the blood into the central ...