This project was funded by R01 DK124509 from NIDDK.

All mice used and the protocols described in this study were in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals, and the Institutional Animal Use and Care Committee at the University of Nevada, Reno, NV. Experiments and animal use also conformed to the principles and regulations as described by Grundy28.
1. Generate PDGFR&#945;-GCaMP6f and SMCGCaMP3 mice
<ol>
	<li>Cross GCaMP6flox/+ mice (B6; 129S-Gt(ROSA)26Sortm95.1(CAG-GCaMP6f)Hze/J) with PDGFR&#945;Cre mice (C57BL/6-Tg(Pdgfra-cre)1Clc/J) to generate PDGFR&#945;-GCaMP6f mice.</li>
	<li>Cross GCaMP3lox/+ mice (B6.129S-Gt(ROSA)26Sortm38(CAG-GCaMP3)Hze/J) with male smMHCCreERT2 mice (B6.FVB-Tg(Myh11-cre/ERT2)1Soff/J) to generate SMC-GCaMP3 mice. 
	NOTE: Only male mice of the cross (GCaMP3lox/+ mice and smMHCCreERT2 mice) can be used as Cre expression is driven from the Y chromosome. smMHCCreERT2 mice can also be crossed with GCaMP6flox/+ mice for improved Ca2+ signal-to-noise ratio and faster Ca2+ signal temporal properties.</li>
</ol>
2. Prepare and inject transgenic mice with tamoxifen to induce conditional expression of GCaMP
<ol>
	<li>Activate inducible Cre recombinase for cell-specific GCaMP expression in specific cell types, as previously described29.</li>
</ol>
3.&#160;Prepare solutions
<ol>
	<li>Prepare 1 L of Krebs-Ringer bicarbonate (KRB) solution containing 120.35 mM NaCl, 5.9 mM KCl, 15.5 mM NaHCO3, 1.2 mM Na2HPO4,1.2 mM MgCl2, 11.5 mM glucose, and 2.5 mM CaCl2. On the day of use, maintain the KRB solution on ice. 
	NOTE: KRB can be stored at 4 &#176;C for up to one week and should be pre-bubbled with a mix of 97% O2 and 3% CO2 for at least 10 min prior to use.</li>
</ol>
4. Prepare silicon elastomer-coated dissection and microscope imaging dishes
<ol>
	<li>Mix silicon elastomer components according to the manufacturer&#39;s instructions. Fill a 35 mm x 10 mm Petri dish and a 60 mm x 15 mm Petri dish approximately one-fourth full of liquid silicon elastomer for imaging experiments and dissection, respectively. Polymerize the silicon elastomer at 37 &#176;C for 1 day prior to use. 
	&#8203;NOTE: To enhance the contrast of thin kidney sections, apply a small, black circle of paper to the base of the imaging Petri dish before filling with silicon elastomer.</li>
</ol>
5. Kidney dissection
<ol>
	<li>Anaesthetize mice by inhalation of 3-4% isoflurane in a ventilated hood. Confirm the induction of deep anesthesia by loss of toe and/or tail pinch reflex, and then euthanize the mice by cervical dislocation.</li>
	<li>Apply 70% ethanol to the chest to dampen the fur. Using external dissection scissors, open the abdominal cavity via a longitudinal incision, with scissor blades angled away from the animal to prevent damage to the internal organs.</li>
	<li>Using internal tissue forceps and internal dissection scissors, pinch the intestines and lift them away from the abdominal wall. Whilst lifting the intestines, cut the underside of the intestines free from the body at the proximal duodenum and distal colon to gain access to the retroperitoneal space containing the kidneys.</li>
	<li>Once the kidneys are exposed, extract them individually. Gently pinch and lift the distal end of the ureter (~4mm away from the kidney) with tissue forceps. Using the dissection scissors, cut underneath the pinched ureter towards the kidney. Continue to cut underneath the kidney until it has become liberated from the surrounding connective tissue. 
	NOTE: To maximize tissue integrity and cutting consistency during vibratome sectioning, the kidney must be as intact as possible. To ensure this, avoid pinching or cutting of the kidney with forceps and dissection scissors.</li>
	<li>Place the kidney with attached ureter in ice-cold KRB solution. Repeat steps 5.4 and 5.5 with the contralateral kidney. Maintain the kidneys in KRB solution on ice. 
	&#8203;NOTE: Immediately proceed to the next section of the protocol to preserve PKJ tissue viability. Because of its anatomical location deep in the kidney parenchyma, the PKJ is deprived of contact with KRB solution.</li>
</ol>
6. Prepare the kidney for vibratome sectioning
<ol>
	<li>Transfer the kidney to a silicon elastomer-coated dissection dish (60 mm x 15 mm), and fill it with ice-cold KRB solution until the kidney is completely submerged.</li>
	<li>Under a dissecting microscope, anchor the kidney to the base of the dish by inserting minutien pins into the proximal ureter and through the thin anterior renal capsule or surrounding adipose tissue. 
	NOTE: Take care not to puncture the kidney parenchyma tissue.</li>
	<li>Use fine spring scissors and internal forceps to remove adipose tissue from the base of the kidney to expose the distal RP and proximal ureter.</li>
	<li>Remove the proximal ureter and a portion of the distal RP from the base of RP using fine spring scissors. 
	NOTE: Take care not to cut the surrounding kidney parenchyma. The black dashed line in Figure 1A indicates the approximate position of this cut. This cut creates a flat base on the kidney for more uniform tissue sectioning. When dissecting the kidney, one must be aware of the anatomical position of the PKJ region. Figure 1B shows that the intact kidney can be cut along a sagittal plane to expose the medulla, papilla (distal medulla where collecting ducts converge) and proximal and distal RP. If the papilla were to be exposed completely, as in Figure 1C, the PKJ and proximal RP (prox RP) can be visualized. However, this should not be done for the vibratome technique; this description is to orientate the reader to the PKJ location generally, emphasized in the anatomical difference shown in the transmitted light images of the PKJ region and mid-RP region in Figure 1D,E.</li>
	<li>Pierce the outer renal capsule with fine-tip forceps, angling the tips away from the kidney body. Using forceps with each hand, pinch the loose ends of the capsule and peel them apart. Continue to peel back the remaining renal capsule membrane until it is removed entirely. 
	&#8203;NOTE: The renal capsule is a tough, fibrous layer that surrounds the kidney. It must be removed prior to vibratome sectioning for optimal cutting.</li>
</ol>
7. Prepare and calibrate the vibratome instrument
<ol>
	<li>Insert a razor blade into the blade holder of the vibratome instrument, and adjust the blade clearance angle to ~18&#176;. 
	NOTE: As an optional step for higher quality sectioning, a calibration block (provided with some vibratome instruments) should be used to adjust the blade position for each new blade used according to the manufacturer&#39;s instructions. This will ensure optimum positioning of the blade and minimize vertical vibration.</li>
	<li>Adjust the blade advancement speed to 0.2 mm/s, the horizontal vibration/sheering of the blade to an amplitude of 2.00 mm, and the Z-step size of the blade to ~100-150 &#181;m. Ensure that kidney section thickness does not exceed 150 &#181;m as this will negatively impact Ca2+ imaging experiments (because the PKJ wall will often roll and fold on itself if it is too thick). 
	NOTE: The user should fine-tune these cutting parameters because settings will vary between individual kidney preparations and vibratome instruments. Fine-tuning should take place during sectioning when the user can visually inspect sections under a microscope, as described in step 7.2.</li>
	<li>Install an ice bath and buffer tray onto the vibratome instrument. Fill the ice bath with crushed ice, and fill the inner stage area with ice-cold KRB solution (fill to approximately half-full). During vibratome sectioning, monitor and replace the crushed ice that has melted.</li>
</ol>
8. Vibratome sectioning the kidney
<ol>
	<li>Use blunt-ended forceps to gently grasp and remove the prepared kidney from ice-cold KRB solution. Immediately place the kidney on absorbent paper for ~2-4 s to remove excess external moisture. Gently roll the kidney across the absorbent paper to ensure that all sides of the parenchyma have dried so that there is optimal adhesion of the kidney to the vibratome stage. 
	NOTE: As the RP is located inside the kidney and therefore protected by the outer parenchyma, this short drying period would not be detrimental to tissue integrity.</li>
	<li>Immediately apply a thin layer of cyanoacrylate glue (~1 cm2) to the base of the vibratome specimen plate, and use blunt-ended forceps to place the kidney, ureter side down, on the area covered in glue. Gently apply downward pressure to the top of the kidney with the flat edge of the forceps for approximately 10-20 s to dry the glue. 
	NOTE: To stabilize the kidney during this procedure, use an additional pair of forceps to keep the kidney upright as the glue dries. It is critical that the kidney adheres to the specimen plate in an upright position so that sections are cut straight. To ensure that the kidney has successfully adhered to the specimen plate, gently push the side of the kidney. If the kidney has successfully adhered to the plate, the base of the kidney should stay secured to the plate.</li>
	<li>Firmly secure the specimen plate to the bottom of the buffer tray. Adjust the level of KRB solution so that the top of the kidney is fully immersed. During sectioning steps, as the vibratome blade moves deeper into the buffer tray, remove KRB solution so that the blade holder does not become immersed in solution. 
	NOTE: If the glue has not completely dried before proceeding with this step, the glue will often move up from the base and on to the kidney parenchyma. This excess glue will make sectioning more variable. If this does happen, remove the kidney from the plate and proceed with a fresh kidney preparation.</li>
	<li>For automatic vibratome sectioning, select the start and end positions of the vibratome blade-cutting cycle. Verify these positions are ~0.5-1 cm clear of the kidney to ensure that with each blade advancement, the entire kidney plane is sectioned.</li>
	<li>Prepare a multi-welled plate (24- or 48-well) by filling wells with KRB solution and place the plate on ice. 
	NOTE: When generated, individual sections should be placed into separate wells to keep track of section depth.</li>
	<li>Start the automatic cutting process. During the initial pass of the blade, ensure that the blade makes contact with the very top of kidney. If contact is not made, adjust the starting Z-position of the blade.</li>
	<li>Using forceps, collect sections that are liberated from the kidney. Immediately transfer the sections to individual wells, and note the Z-depth of the sections to gauge the approximate PKJ location within kidney sections. 
	NOTE: Depending on the cut parameters, some sections may not be cut free from the kidney block. If this occurs, carefully use fine spring scissors to cut sections from the kidney block. Users are also encouraged to actively visualize sections under a light microscope whilst free-floating in individual wells to ensure optimal cut settings and tissue location. Sections containing the PKJ will typically be derived ~ 1000-1500 &#181;m from the top of the kidney.</li>
	<li>Continue the sectioning protocol until the PKJ regions become more apparent. Refer to the representative results section for description of the PKJ regions as sectioning proceeds.</li>
	<li>At this point, optimize the sectioning parameters to ensure that sections are liberated from the kidney block uniformly and are intact. Additionally, make sure that the PKJ regions are continuous and unbroken because broken PKJ walls will not allow adequate imaging of cells within the wall due to collapse. If walls become broken, decrease the sectioning speed and increase the section thickness, and continue to observe sections under a light microscope to fine-tune the cutting parameters.</li>
	<li>Store sections at 4&#176;C in KRB solution until experimentation begins.</li>
</ol>
9. Kidney slice Ca2+ image acquisition
<ol>
	<li>Transfer an individual kidney slice to a silicon elastomer-coated imaging dish (35 mm x 10 mm), and immediately fill the dish with fresh, ice-cold KRB solution.</li>
	<li>Insert minutien pins around the periphery of a kidney slice to secure the section to the base of the imaging dish. 
	NOTE: This step is critical to prevent the section from moving around when physiological solutions are perfused over the slice during imaging.</li>
	<li>Place the imaging dish on the stage of an upright spinning-disk confocal microscope and immediately start perfusing with KRB solution. 
	NOTE: In this protocol, an upright microscope equipped with a high-speed Nipkow spinning disk confocal scanner unit was used.</li>
	<li>Maintain the perfusion rate at 3 mL/min and KRB solution temperature at 36 &#177; 1 &#176;C. Prior to imaging, allow the slice to equilibrate for 1 h.</li>
	<li>Select the appropriate dichroic imaging cube and lasers. Acquire images with an electron-multiplying charge-coupled device (EMCCD) or scientific complementary metal-oxide-semiconductor camera. 
	NOTE: The confocal system in this protocol is equipped with a 488 nm laser to excite GCaMP6f or GCaMP3. Images were acquired using a 512 pixel x 512 pixel EMCCD camera.</li>
	<li>Use a low magnification, water-immersion objective lens (4x or 10x) to locate the kidney slice. Center the imaging field on areas of the slice where the PKJ is present. Identify landmarks, as depicted in Figure 2D, to locate the PKJ (i.e., semicircles of muscular tissues suspended between parenchymal tissue).</li>
	<li>Once the PKJ is located, use a higher magnification water-immersion objective lens (20x, 40x, or 60x) to magnify the area of interest. 
	NOTE: In this protocol, the 20x objective numerical aperture (NA) was 1.0, the 40x objective NA was 0.8, and the 60x objective NA was 1.0.</li>
	<li>Distinguish different cells of interest in the PKJ wall using transgenic mice expressing GCaMP6f or GCaMP3 in PDGFR&#945;+ cells or SMCs, respectively. Observe the different types of Ca2+ transient durations in PDGFR&#945;+ cells in the PKJ wall in PDGFR&#945;+ GCaMP6f+ kidney slices (Figure 3C, see representative results for description) and in GCaMP3+ SMCs in SMC GCaMP3+ kidney slices (Figure 3D, see representative results for description).</li>
	<li>Once cells of interest in PKJ wall have been identified, adjust the laser intensity to yield a good signal-to-noise ratio. Record images at a temporal sampling frequency between 16 Hz and 32 Hz using appropriate acquisition software. 
	NOTE: Depending on laser intensity used during imaging, it is recommended to limit the number of recordings owing to the bleaching effects on Ca2+ fluorophores. The user should choose recording length based upon the specific experimental objectives.</li>
</ol>
10. Ca2+ imaging analysis
<ol>
	<li>Perform Ca2+ imaging analysis of different cell types in PKJ pacemaker regions by spatiotemporal mapping as previously described for other intact pacemaker preparations in the gastrointestinal tract29,30.</li>
</ol>

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M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Applications+of+spatio-temporal+mapping+and+particle+analysis+techniques+to+quantify+intracellular+Ca+2++signaling+in+situ.">Applications of spatio-temporal mapping and particle analysis techniques to quantify intracellular Ca 2+ signaling in situ.</a> Journal of Visualized Experiments. 2019 (143), 1-13 (2019).</li><li>Leigh, W. A., 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+high+throughput+machine-learning+driven+analysis+of+Ca2++spatio-temporal+maps.">A high throughput machine-learning driven analysis of Ca2+ spatio-temporal maps.</a> Cell Calcium. 91, 102260 (2020).</li></ol>

The authors have nothing to disclose.

The RP consists of a heterogeneous population of cells with differential cell densities observed in various RP regions. PIC1s (previously referred to as ASMCs) are most abundant in the PKJ, where pacemaker activity originates24. The protocol, described here, allows investigators to isolate the pacemaker region from the rest of the mouse kidney. By cutting sections of PKJ using a vibratome, the pacemaker regions of the RP (identified as muscle bands attached to parenchyma) are kept intact, thus affording the use of in situ imaging to accurately study RP pacemaker cells when combined with cell-specific fluorescence reporters.
While this approach can provide new insights into RP pacemaking, there are some considerations that experimenters should be familiar with to improve imaging outcomes and sectioning efficiency. For an untrained user, this method of PKJ isolation and imaging is easier to learn than typical sharp dissection of flat-sheet RP preparations. Sharp dissection of RP from whole kidneys requires weeks of consistent practice to successfully isolate viable tissues for physiology experiments. As this vibratome sectioning protocol requires little sharp dissection knowledge, it is accessible to users who do not have experience dissecting other smooth muscle structures.
However, there are some critical points to note for this protocol. Successfully adhering kidneys to the vibratome specimen plate requires dexterity and patience. If the kidney is orientated incorrectly and leans to one side, oblique rather than straight sections will be cut. Due to the delicate nature of the PKJ, the oblique angle can often destroy the muscle bands of the pacemaker region. Furthermore, imaging of oblique sections results in poor imaging acquisition as cell networks are not typically in the same focal plane. The procedure is also time-consuming, with sectioning of a single kidney often taking up to an hour to complete, during which time the setup requires monitoring.
While the movement of the vibratome can be sped up, if the speed is increased too much (&#62;20% than what is recommended in the protocol), the blade will shred rather than cleanly cut the kidney, resulting in loss of delicate PKJ structures. Similarly, a cutting speed that is too low can cause the section to become jagged. Optimization of cutting speed and blade amplitude is essential. Care must also be taken in handling vibratome sections. Due to their delicate nature, PKJ muscles are easily disrupted during handling and can tear. A well-trained user will be able to harvest approximately 1-2 PKJ regions per 4 kidney slices that are suitable for Ca2+ imaging experiments. Typically, PKJ sections that do not meet Ca2+ imaging criteria have: 1) poor GCaMP expression, 2) a contorted PKJ wall, or 3) a broken PKJ wall. For data analysis, approximately 3-4 cells per field of view (FOV) could be sampled.
Whilst there are many cells in the FOV of PDGFR&#945;-GCaMP6f and SMC-GCaMP3 PKJ sections, small tissue movements often exclude cells from analysis. This can usually be resolved by applying a stabilization protocol to images. Under conditions where preparations do not move, at least 3-5 cells can be sampled from PDGFR&#945;-GCaMP6f sections and 5-6 cells from SMC-GCaMP3 sections. Typically, the time taken from animal sacrifice (optimum age for mice is 8-16 weeks) to performing Ca2+ imaging experiments is 2-3 h, which is adequate to ensure tissue integrity, if tissues are incubated in ice-cold solutions throughout the procedure when required. In summary, a vibratome cutting protocol has been described here to generate intact preparations of RP PKJ regions from the mouse kidney. This technique allows the preservation of RP pacemaker regions for in situ Ca2+ imaging studies to investigate RP pacemaker mechanisms.

The renal pelvis (RP) is a funnel-shaped, smooth muscle structure that transports urine from the kidney to the ureter. The RP transports urine by generating regular rhythmic contractions (peristalsis)1,2,3,4,5, which propels a bolus of urine from the kidney distally to the ureter and ultimately to the bladder, where it is stored until micturition occurs6,7. Loss of this regular activity has dire consequences, including hydronephrosis and kidney failure1,3,8; hence, there is a critical need to study the mechanisms underlying regular, rhythmic RP contractions. Peristaltic contractions originate from the most proximal region of the RP-in the pelvis-kidney junction (PKJ)9,10,11,12,13,14,15 (Figure 1A-C) and propagate distally to push urine from the papilla into the RP (Figure 1B). Electrical pacemaker activity is recorded in the PKJ as spontaneous transient depolarizations10,11,12,13,15,16,17, which are thought to arise from specialized pacemaker cells. These pacemaker cells, previously called atypical smooth muscle cells (ASMCs), are thought to generate or coordinate pacemaker activity and drive the contractions of &#34;typical&#34; smooth muscle cells (SMCs)9,10,11,18,19,20,21,22,23.
ASMCs are most abundant in the proximal RP, at the PKJ (Figure 1A-C), where peristaltic contractions and electrical pacemaker activity originates5,7,8,9,12,13,14,16,17,18,19,20,21,22. A recently published study by this group identified platelet-derived growth factor receptor-alpha (PDGFR&#945;), in combination with smooth muscle myosin heavy chain (smMHC), as a unique biomarker for these interstitial cells (ICs)24, a finding that has been corroborated by other groups25. Based on their morphology and protein expression pattern, these cells were called PDGFR&#945;+ IC type 1 (PIC1)24,26. PIC1s reside in the muscle layer of the PKJ where they display high-frequency, short-duration Ca2+ transients, thought to underlie the generation of pacemaker potentials24. However, other cell types exist in the PKJ, including non-smMHC-expressing PDGFR&#945;+ ICs (PIC2s) in the adventitial layer. Previous reports have suggested that non-smMHC ICs may participate in the regulation of pacemaker activity19. However, further study of non-smMHC ICs is hindered by poor distinction during Ca2+ imaging studies. Typically, heterogeneous cell types within the RP preparations are indiscriminately loaded with Ca2+-sensitive dyes (e.g., Fluo-4). To overcome these challenges and to study a variety of cell types in the RP, genetically encoded Ca2+ indicators (GECIs) can be utilized to selectively express Ca2+-sensitive fluorophores in cell types of interest.
The majority of studies elucidating Ca2+ transient properties in PIC1s/ASMCs were achieved by imaging flat-sheet RP tissue preparations19,21,27. As PIC1s are the only cell type in the PKJ to express smMHC, conditional expression of the GECI, GCaMP, in smMHC+ cells is appropriate to study PIC1s in this configuration. However, as PIC1s and PIC2s both express PDGFR&#945;, conditional expression of GCaMP variants in PDGFR&#945;+ cells prohibit cell distinction in flat-sheet preparations. To circumvent this issue, a vibratome sectioning approach was used to distinguish PIC1s and PIC2s across the PKJ tissue wall24. To reveal these discrete cellular populations, the RP was sectioned coronally, making it possible to identify PIC2s in the adventitia and PIC1s in the muscle wall based on known immunohistochemical labeling and GECI expression patterns. As a result of this novel PKJ imaging approach, PIC1s and PIC2s were found to display distinct Ca2+ signaling properties24. Furthermore, by isolating the most proximal sections of the PKJ region (Figure 2), the pacemaker region of the RP was preserved in a way that had not been accomplished previously. Here, a protocol is described to show how to isolate PKJ preparations from the mouse kidney using vibratome sectioning, how to set up these preparations for Ca2+ imaging experiments, and how to distinguish the different cell types across the PKJ wall.

<table><tbody><tr><td>24-well culture plate</td><td>ThermoFisher Scientific</td><td>142485</td><td>To store kidney slices in</td></tr><tr><td>35 mm x 10 mm Petri dishes</td><td>Sigma Aldrich</td><td>CLS430165</td><td>Kidney slice calcium imaging dish</td></tr><tr><td>48-well culture plate</td><td>ThermoFisher Scientific</td><td>152640</td><td>To store kidney slices in</td></tr><tr><td>60 mm x 15 mm Petri dish</td><td>Sigma Aldrich</td><td>P5481</td><td>Kidney sharp dissection dish</td></tr><tr><td>Absorbent paper</td><td>Fisher Scientific</td><td>06-666A</td><td>To dry the kidney before applying glue</td></tr><tr><td>B6;129S-Gt(ROSA)26Sor/J</td><td>The Jackson Laboratory</td><td>13148</td><td>GCaMP3 Mice</td></tr><tr><td>B6;129S-Gt(ROSA)26Sor/J</td><td>The Jackson Laboratory</td><td>24105</td><td>GCaMP6f Mice</td></tr><tr><td>B6.FVB-Tg(Myh11-cre/ERT2)1Soff/J</td><td>The Jackson Laboratory</td><td>19079</td><td>smMHC-CRE Mice</td></tr><tr><td>C57BL/6-Tg(Pdgfra-cre)1Clc/J</td><td>The Jackson Laboratory</td><td>13148</td><td>PDGFRa-CRE Mice</td></tr><tr><td>Cyanoacrylate glue</td><td>Amazon</td><td>B001PILFVY</td><td>For adhering the kidney to the specimen plate</td></tr><tr><td>Ethanol</td><td>Phamco-Aaper</td><td>SDA 2B-6</td><td>For dissection</td></tr><tr><td>Extra-Fine Bonn Scissors</td><td>Fine Science Tools</td><td>14083-08</td><td>Used for internal dissecting scissors</td></tr><tr><td>Fine scissors</td><td>Fine Science Tools</td><td>14060-09</td><td>Used for external dissecting scissors</td></tr><tr><td>Fine-tip forceps</td><td>Fine Science Tools</td><td>11254-20</td><td>Used for fine dissection of kidney</td></tr><tr><td>Gillette Silver Blue double-edge blades</td><td>Amazon</td><td>B009XHQGYO</td><td>For insertion into blade holder of vibratome</td></tr><tr><td>ImageJ</td><td>NIH</td><td></td><td>For calcium imaging analysis</td></tr><tr><td>Isoflurane</td><td>Baxter</td><td>NDC 1001936060</td><td>For anesthesia</td></tr><tr><td>Minutien pins</td><td>Fisher Scientific</td><td>NC9677548</td><td>Pins were cut in half to reduce their length</td></tr><tr><td>Silicon elastomer</td><td>Fisher Scientific</td><td>NC9285739</td><td>Sylgard 184</td></tr><tr><td>Student Adson Forceps</td><td>Fine Science Tools</td><td>91106-12</td><td>For gently holding and moving the kidney</td></tr><tr><td>Student Dumont Forceps</td><td>Fine Science Tools</td><td>91150-20</td><td>Used for internal dissecting forceps</td></tr><tr><td>Vannas spring scissors</td><td>Fine Science Tools</td><td>15000-03</td><td>For sharp dissection and cleanup of isolated kidney</td></tr><tr><td>Vibrocheck</td><td>Leica</td><td>14048142075</td><td>Optional component for calibrating blade movement during cutting</td></tr><tr><td>VT1200 S Vibrating Blade Microtome</td><td>Leica</td><td>14912000001</td><td>Configuration 1 is used in our protocol</td></tr></tbody></table>

isolating and imaging live, intact pacemaker regions of mouse renal pelvis by vibratome sectioning

The renal pelvis (RP) is a funnel-shaped, smooth muscle structure that facilitates normal urine transport from the kidney to the ureter by regular, propulsive contractions. Regular RP contractions rely on pacemaker activity, which originates from the most proximal region of the RP at the pelvis-kidney junction (PKJ). Due to the difficulty in accessing and preserving intact preparations of the PKJ, most investigations on RP pacemaking have focused on single-cell electrophysiology and Ca2+ imaging experiments. Although important revelations on RP pacemaking have emerged from such work, these experiments have several intrinsic limitations, including the inability to accurately determine cellular identity in mixed suspensions and the lack of in situ imaging of RP pacemaker activity. These factors have resulted in a limited understanding of the mechanisms that underlie normal rhythmic RP contractions. In this paper, a protocol is described to prepare intact segments of mouse PKJ using a vibratome sectioning technique. By combining this approach with mice expressing cell-specific reporters and genetically encoded Ca2+ indicators, investigators may be able to more accurately study the specific cell types and mechanisms responsible for peristaltic RP contractions that are vital for normal urine transport.

In situ Ca2+ imaging of the PKJ can reveal important cellular activity of RP pacemaker cells. By using mice that express genetically encoded Ca2+ indicators (such as GCaMP), driven by cell-specific promotors, information about RP pacemaking can be obtained with accuracy and detail that is not possible from Ca2+ imaging experiments from flat-sheet RP preparations. The beginning of the PKJ is distinguished by the sudden appearance of semi-circles of muscle suspended between kidney parenchymal tissue (Figure 2C; proximal PKJ enclosed in dashed box). During subsequent rounds of sectioning, the inner medulla becomes distinguishable from the surrounding cortical tissue. Under a light microscope, the inner medulla appears striated in regions, lighter in color compared to cortical tissue and discontinuous on its long axis with the rest of the kidney (Figure 2B,D). At this point, more PKJ regions will start to appear. Examples of this are shown in Figure 2D (dashed rectangles, H and G) where 3 semi-circles of muscle are suspended by parenchymal tissue. These muscle bands will be closely apposed to the inner papilla and will typically neighbor a renal arteriole (Figure 2D, dashed rectangles; Figure 2F-H, black arrowheads). As more distal sections are derived, these bands of muscle will integrate to form a more complete, unified structure, indicating the end of the PKJ region (Figure 2E). 
Figure 3A,B shows a PKJ section at low power (4-10x) from a mouse expressing GCaMP in PDGFR&#945;+ cells (GCaMP6f expressed by inducible Cre-recombinase driven by Pdgfra). Using landmarks such as the renal arteriole (Figure 3A; asterisk), experimenters should be able to readily distinguish the thin PKJ wall suspended between parenchymal tissue (Figure 3B; asterisks). The expression of GCaMP6f in this specific transgenic tissue is spread across the entire width of the PKJ, across both the muscle and adventitial layers (Figure 3C).
In PDGFR&#945;+ GCaMP6f+&#160;kidney slices, a network of cells that typically extends over the width of the PKJ wall will be fluorescent (Figure 3C) and display oscillating Ca2+ transients of various durations and frequencies. PDGFR&#945;+ cells in the PKJ wall display two different types of Ca2+ transient durations. In the adventitial layer (orientated closer to cortex), PDGFR&#945;+ cells present as a network of cells and their processes are defined. Adventitial PDGFR&#945;+ cells exhibit low-frequency (4 &#177; 2.7 Hz) and long-duration (1 &#177; 0.67 s) Ca2+ transients. The second layer of PDGFR&#945;+ cells, present in the muscle layer (orientated closer to the medulla), exhibit similar Ca2+ transient frequencies and durations as SMC GCaMP3+ cells (described below) as they are the same cell type.
In SMC GCaMP3+ kidney slices, a layer of GCaMP3+ cells is present in the muscle layer (Figure 3D). There will be no fluorescent signal in the adventitial layer (Figure 3D; asterisk). GCaMP3+ SMCs in the muscular layer typically exhibit high-frequency (10 &#177; 4 Hz) and short-duration (632 &#177; 74 s) Ca2+ transients. PDGFR&#945;+ cells located in the PKJ adventitia elicit long-duration, low-frequency Ca2+ transients (Figure 3E, Video 1). However, Ca2+ imaging experiments from tissue expressing GCaMP3 driven by the Myh11 promotor is restricted to the muscular aspect of the PKJ (Figure 3D). Compared to PDGFR&#945;+ cells in the adventitia, SMCs fired shorter duration Ca2+ transients more frequently (Figure 3F, Video 2).
In addition to understanding signaling properties in PKJ PDGFR&#945;+ ICs, the application of this technique to study other cell types in the vibratome-sectioned kidney has been demonstrated in this paper. Upon close examination of the renal medulla (in mice expressing GCaMP6f in PDGFR&#945;+ cells), an array of fluorescent Ca2+ signals within and surrounding collecting ducts (Video 3) was observed. Medullary PDGFR&#945;+ cells fired spontaneous Ca2+ transients of variable frequency and duration. These Ca2+ imaging studies of kidney vibratome sections could also be expanded to studying renal arterioles (~50-80 mm diameter) that often neighbor PKJ muscle segments (Figure 2F,G; white arrows). Ca2+ imaging of renal arterioles (from tissue expressing GCaMP in smooth muscle cells) demonstrates oscillating Ca2+ transients in SMCs (Video 4).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/62040/62040fig01.jpg" /> 
Figure 1: Basic kidney anatomy and location of PKJ pacemaker region. (A) Diagram of the intact kidney showing the orientation of the RP and ureter. The renal artery and renal vein are displayed in red and blue, respectively. (B) The intact kidney can be cut along a sagittal plane to expose the inner aspect of the kidney, including the medulla, papilla (distal medulla where collecting ducts converge), and proximal and distal RP. (C) The medulla and papilla can be excised to completely expose the PKJ and prox RP. (D and E) represent transmitted light images from the PKJ pacemaker region and distal RP, respectively. Sequential sectioning towards the distal end of the pelvis results in the semicircles of muscle in the PKJ region (Di) combining into one, thicker muscular ring (Ei) that encapsulates the entire papilla. Black, dashed rectangles in Di and Ei show approximate areas in coronal kidney sections where transmitted light images were acquired. Orientation of images D and E are 90&#176; anti-clockwise to respective insets (Di and Ei). Scale bars in D and E = 20 &#181;m. Abbreviations: RP = renal pelvis; prox RP = proximal renal pelvis; PKJ = pelvic-kidney junction; PICs = platelet-derived growth factor receptor-alpha-positive interstitial cells; SMC = smooth muscle cell. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/62040fig01large.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/62040/62040fig02.jpg" /> 
Figure 2: Vibratome sectioning of whole kidneys to generate thin sections. (A)&#160;Kidneys are mounted ureter side down to the base of the vibratome instrument, and a standard blade (attached to the vibratome head) is used to cut sequential sections from the proximal to distal end of the kidney. (B) Diagrammatic representation of a thin section cut from the whole kidney with annotated landmarks. PKJ muscle segments (black dashed rectangle) are often found suspended between parenchymal tissue. (C) Light microscopic image of a proximal kidney section. The appearance of muscle bands suspended between parenchymal tissue indicates the beginning of the proximal PKJ projections (indicated inside white dashed rectangle). (D) Light microscopic image representing the optimal region where multiple (2-3) PKJ segments can be found (areas within white dashed rectangles). Thin PKJ muscle strips are suspended between the kidney parenchyma and align closely with renal arterioles and medulla. (E) Light microscopic image of a distal kidney section. Individual muscle segments have merged to form a single, continuous muscle band (white dashed rectangle) that surrounds the inner papilla (not present in this image). Scale bars C-E = 500 &#181;m. F-H Zoomed (20x) regions from panel D indicate the location of the PKJ (black arrowheads), renal arterioles (white arrowheads), and cut sites for isolating the PKJ (dashed white lines). Scale bars F-H = 100 &#181;m. Abbreviation: PKJ = pelvic-kidney junction. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/62040fig02large.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/62040/62040fig03.jpg" /> 
Figure 3: Ca2+ imaging of vibratome sections. (A) Representative low-power image (4x) of a vibratome section denoting location of the renal arteriole (asterisk). Scale bar = 200 &#181;m. (B) Zoomed (20x) representative image of the PKJ (labeled) suspended between kidney parenchymal tissue denoting locations of the PKJ muscle (white arrowhead), renal arteriole (asterisk). Scale bar = 50 &#181;m. (C) High-power (40x) image of the PKJ expressing GCaMP in PDGFR&#945;+ cells. Scale bar = 20 &#181;m. (D) High-power (20x) image of the PKJ expressing GCaMP in smooth muscle cells. Scale bar = 20 &#181;m. (E) Spatiotemporal map of Ca2+ transients sampled from a GCaMP+ PDGFR&#945;+ cell indicated in panel C. Look up table coded for F/F0. (F) Spatiotemporal map of Ca2+ transients sampled from a GCaMP+ PDGFR&#945;+ cell indicated in panel D. Look up table coded for F/F0. (G) Representative data for Ca2+ transient frequency (Hz) for GCaMP+ PDGFR&#945;+ cells and GCaMP+ smMHC cells. (H) Representative data for Ca2+ transient duration (s) for GCaMP+ PDGFR&#945;+ cells and GCaMP+ smMHC cells. Abbreviations: PKJ = pelvic-kidney junction; PDGFR&#945;+ = platelet-derived growth factor receptor-alpha-positive; smMHC = smooth muscle myosin heavy chain. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/62040fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
Video 1: Spontaneous Ca2+ transients in GCaMP+ PDGFR&#945;+ cells in PKJ vibratome sections. Abbreviations: PKJ = pelvic-kidney junction; PDGFR&#945;+ = platelet-derived growth factor receptor-alpha-positive. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/Video_1.avi" target="_blank">Please click here to view this video. (Right-click to download.)</a>
Video 2: Spontaneous Ca2+ transients in GCaMP+ smooth muscle cells in pelvic-kidney junction vibratome sections. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/Video_2.avi" target="_blank">Please click here to view this video. (Right-click to download.)</a>
Video 3: Spontaneous Ca2+ transients in GCaMP+ PDGFR&#945;+ cells in renal medullary vibratome sections. Abbreviation: PDGFR&#945;+ = platelet-derived growth factor receptor-alpha-positive. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/Video_3.avi" target="_blank">Please click here to view this video. (Right-click to download.)</a>
Video 4: Low-amplitude Ca2+ transient activity in the vibratome sections of the renal arteriole. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/62040/Video_4.avi" target="_blank">Please click here to view this video. (Right-click to download.)</a>

Watch this Scientific Journal Video about Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning at JoVE.com

Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning

The goal of this protocol is to isolate intact pacemaker regions of the mouse renal pelvis using vibratome sectioning. These sections can then be used for in situ Ca2+ imaging to elucidate Ca2+ transient properties of pacemaker cells and other interstitial cells in vibratome slices.

The renal pelvis (RP) is a funnel-shaped, smooth muscle structure that facilitates normal urine transport from the kidney to the ureter by regular, ...

isolating-imaging-live-intact-pacemaker-regions-mouse-renal-pelvis

Universidad de Cartagena UDEC

Research

JoVE Journal

Biology

3.2K Views.  University of Nevada, Reno School of Medicine. The goal of this protocol is to isolate intact pacemaker regions of the mouse renal pelvis using vibratome sectioning. These sections can then be used for in situ Ca2+ imaging to elucidate Ca2+ transient properties of pacemaker cells and other interstitial cells in vibratome slices.

Video: Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning

Optical Imaging of Isolated Murine Ventricular Myocytes

The ability to isolate adult cardiac myocytes has permitted researchers to study a variety of cardiac pathologies at the single cell level. While advances in calcium sensitive dyes have permitted the robust optical recording of single cell calcium dynamics, recording of robust transmembrane optical voltage signals has remained difficult. Arguably, this is because of the low single to noise ratio, phototoxicity, and photobleaching of traditional potentiometric dyes. Therefore, single cell voltage measurements have long been confined to the patch clamp technique which while the gold standard, is technically demanding and low throughput. However, with the development of novel potentiometric dyes, large, fast optical responses to changes in voltage can be obtained with little to no phototoxicity and photobleaching. This protocol describes in detail how to isolate adult murine myocytes which can be used for cellular shortening, calcium, and optical voltage measurements. Specifically, the protocol describes how to use a ratiometric calcium dye, a single-excitation calcium dye, and a single excitation voltage dye. This approach can be used to assess the cardiotoxicity and arrhythmogenicity of various chemical agents. While phototoxicity is still an issue at the single cell level, methodology is discussed on how to reduce it.

We present the methodology for the isolation of murine myocytes and how to obtain voltage or calcium traces simultaneously with sarcomere shortening traces using fluorescence photometry with simultaneous digital cell geometry measurements.

The ability to isolate adult cardiac myocytes has permitted researchers to study a variety of cardiac pathologies at the single cell level. While advances ...

Bioengineering

Preclinical Cardiac Electrophysiology Assessment by Dual Voltage and Calcium Optical Mapping of Human Organotypic Cardiac Slices

Human cardiac slice preparations have recently been developed as a platform for human physiology studies and therapy testing to bridge the gap between animal and clinical trials. Numerous animal and cell models have been used to examine the effects of drugs, yet these responses often differ in humans. Human cardiac slices offer an advantage for drug testing in that they are directly derived from viable human hearts. In addition to having preserved multicellular structures, cell-cell coupling, and extracellular matrix environments, human cardiac tissue slices can be used to directly test the effect of innumerable drugs on adult human cardiac physiology. What distinguishes this model from other heart preparations, such as whole hearts or wedges, is that slices can be subjected to longer-term culture. As such, cardiac slices allow for studying the acute as well as chronic effects of drugs. Furthermore, the ability to collect several hundred to a thousand slices from a single heart makes this a high-throughput model to test several drugs at varying concentrations and combinations with other drugs at the same time. Slices can be prepared from any given region of the heart. In this protocol, we describe the preparation of left ventricular slices by isolating tissue cubes from the left ventricular free wall and sectioning them into slices using a high precision vibrating microtome. These slices can then either be subjected to acute experiments to measure baseline cardiac electrophysiological function or cultured for chronic drug studies. This protocol also describes dual optical mapping of cardiac slices for simultaneous recordings of transmembrane potentials and intracellular calcium dynamics to determine the effects of the drugs being investigated.

This protocol describes the procedure for sectioning and culturing human cardiac slices for preclinical drug testing and details the use of optical mapping for recording transmembrane voltage and intracellular calcium signals simultaneously from these slices.

Human cardiac slice preparations have recently been developed as a platform for human physiology studies and therapy testing to bridge the gap between ...

Murine Short Axis Ventricular Heart Slices for Electrophysiological Studies

Murine cardiomyocytes have been extensively used for in vitro studies of cardiac physiology and new therapeutic strategies. However, multicellular preparations of dissociated cardiomyocytes are not representative of the complex in vivo structure of cardiomyocytes, non-myocytes and extracellular matrix, which influences both mechanical and electrophysiological properties of the heart. Here we describe a technique to prepare viable ventricular slices of adult mouse hearts with a preserved in vivo like tissue structure, and demonstrate their suitability for electrophysiological recordings. After excision of the heart, ventricles are separated from the atria, perfused with Ca2+-free solution containing 2,3-butanedione monoxime and embedded in a 4% low-melt agarose block. The block is placed on a microtome with a vibrating blade, and tissue slices with a thickness of 150-400 &#181;m are prepared keeping the vibration frequency of the blade at 60-70 Hz and moving the blade forward as slowly as possible. Thickness of the slices depends on the further application. Slices are stored in ice cold Tyrode&#39;s solution with 0.9 mM Ca2+ and 2,3-butanedione monoxime (BDM) for 30 min. Afterwards, slices are transferred to 37 &#176;C DMEM for 30 min to wash out the BDM. Slices can be used for electrophysiological studies with sharp electrodes or micro electrode arrays, for force measurements to analyze contractile function or to investigate the interaction of transplanted stem cell-derived cardiomyocytes and host tissue. For sharp electrode recordings, a slice is placed into a 3 cm cell culture dish on the heating plate of an inverted microscope. The slice is stimulated with a unipolar electrode, and intracellular action potentials of cardiomyocytes within the slice are recorded with a sharp glass electrode.

Here, we describe the preparation of viable ventricular slices from adult mice and their use for sharp electrode action potential recordings. These multicellular preparations provide a preserved in vivo like tissue structure, which makes them a valuable model for electrophysiological and pharmacological studies in vitro.

Murine cardiomyocytes have been extensively used for in vitro studies of cardiac physiology and new therapeutic strategies. However, multicellular ...

Medicine

Mouse Fetal Whole Intestine Culture System for Ex Vivo Manipulation of Signaling Pathways and Three-dimensional Live Imaging of Villus Development

Most morphogenetic processes in the fetal intestine have been inferred from thin sections of fixed tissues, providing snapshots of changes over developmental stages. Three-dimensional information from thin serial sections can be challenging to interpret because of the difficulty of reconstructing serial sections perfectly and maintaining proper orientation of the tissue over serial sections. Recent findings by Grosse et al., 2011 highlight the importance of three- dimensional information in understanding morphogenesis of the developing villi of the intestine1. Three-dimensional reconstruction of singly labeled intestinal cells demonstrated that the majority of the intestinal epithelial cells contact both the apical and basal surfaces. Furthermore, three-dimensional reconstruction of the actin cytoskeleton at the apical surface of the epithelium demonstrated that the intestinal lumen is continuous and that secondary lumens are an artifact of sectioning. Those two points, along with the demonstration of interkinetic nuclear migration in the intestinal epithelium, defined the developing intestinal epithelium as a pseudostratified epithelium and not stratified as previously thought1. The ability to observe the epithelium three-dimensionally was seminal to demonstrating this point and redefining epithelial morphogenesis in the fetal intestine. With the evolution of multi-photon imaging technology and three-dimensional reconstruction software, the ability to visualize intact, developing organs is rapidly improving. Two-photon excitation allows less damaging penetration deeper into tissues with high resolution. Two-photon imaging and 3D reconstruction of the whole fetal mouse intestines in Walton et al., 2012 helped to define the pattern of villus outgrowth2. Here we describe a whole organ culture system that allows ex vivo development of villi and extensions of that culture system to allow the intestines to be three-dimensionally imaged during their development.

Mouse Fetal Whole Intestine Culture System for Ex Vivo Manipulation of Signaling Pathways and Three-dimensional Live Imaging of Villus Development

Improved imaging technology is allowing three-dimensional imaging of organs during development. Here we describe a whole organ culture system that allows live imaging of the developing villi in the fetal mouse intestine.

Most morphogenetic processes in the fetal intestine have been inferred from thin sections of fixed tissues, providing snapshots of changes over ...

Whole-Mount Immunofluorescence Staining, Confocal Imaging and 3D Reconstruction of the Sinoatrial and Atrioventricular Node in the Mouse

The electrical signal physiologically generated by pacemaker cells in the sinoatrial node (SAN) is conducted through the conduction system, which includes the atrioventricular node (AVN), to allow excitation and contraction of the whole heart. Any dysfunction of either SAN or AVN results in arrhythmias, indicating their fundamental role in electrophysiology and arrhythmogenesis. Mouse models are widely used in arrhythmia research, but the specific investigation of SAN and AVN remains challenging.
The SAN is located at the junction of the crista terminalis with the superior vena cava and AVN is located at the apex of the triangle of Koch, formed by the orifice of the coronary sinus, the tricuspid annulus, and the tendon of Todaro. However, due to the small size, visualization by conventional histology remains challenging and it does not allow the study of SAN and AVN within their 3D environment.
Here we describe a whole-mount immunofluorescence approach that allows the local visualization of labelled mouse SAN and AVN. Whole-mount immunofluorescence staining is intended for smaller sections of tissue without the need for manual sectioning. To this purpose, the mouse heart is dissected, with unwanted tissue removed, followed by fixation, permeabilization and blocking. Cells of the conduction system within SAN and AVN are then stained with an anti-HCN4 antibody. Confocal laser scanning microscopy and image processing allow differentiation between nodal cells and working cardiomyocytes, and to clearly localize SAN and AVN. Furthermore, additional antibodies can be combined to label other cell types as well, such as nerve fibers.
Compared to conventional immunohistology, whole-mount immunofluorescence staining preserves the anatomical integrity of the cardiac conduction system, thus allowing the investigation of AVN; especially so into their anatomy and interactions with the surrounding working myocardium and non-myocyte cells.

We provide a step-by-step protocol for whole-mount immunofluorescence staining of the sinoatrial node (SAN) and atrioventricular node (AVN) in murine hearts.

The electrical signal physiologically generated by pacemaker cells in the sinoatrial node (SAN) is conducted through the conduction system, which includes ...

Implementing Patch Clamp and Live Fluorescence Microscopy to Monitor Functional Properties of Freshly Isolated PKD Epithelium

Cyst initiation and expansion during polycystic kidney disease is a complex process characterized by abnormalities in tubular cell proliferation, luminal fluid accumulation and extracellular matrix formation. Activity of ion channels and intracellular calcium signaling are key physiologic parameters which determine functions of tubular epithelium. We developed a method suitable for real-time observation of ion channels activity with patch-clamp technique and registration of intracellular Ca2+ level in epithelial monolayers freshly isolated from renal cysts. PCK rats, a genetic model of autosomal recessive polycystic kidney disease (ARPKD), were used here for ex vivo analysis of ion channels and calcium flux. Described here is a detailed step-by-step procedure designed to isolate cystic monolayers and non-dilated tubules from PCK or normal Sprague Dawley (SD) rats, and monitor single channel activity and intracellular Ca2+ dynamics. This method does not require enzymatic processing and allows analysis in a native setting of freshly isolated epithelial monolayer. Moreover, this technique is very sensitive to intracellular calcium changes and generates high resolution images for precise measurements. Finally, isolated cystic epithelium can be further used for staining with antibodies or dyes, preparation of primary cultures and purification for various biochemical assays.

Ion channels expressed in renal tubular epithelium play a significant role in the pathology of polycystic kidney disease. Here we describe experimental protocols used to perform patch-clamp analysis and intracellular calcium level measurements in cystic epithelium freshly isolated from rodent kidneys.

Cyst initiation and expansion during polycystic kidney disease is a complex process characterized by abnormalities in tubular cell proliferation, luminal ...

Preparation of Human Myocardial Tissue for Long-Term Cultivation

Cardiomyocyte cultivation has seen a vast number of developments, ranging from two-dimensional (2D) cell cultivation to iPSC derived organoids. In 2019, an ex vivo way to cultivate myocardial slices obtained from human heart samples was demonstrated, while approaching in vivo condition of myocardial contraction. These samples originate mostly from heart transplantations or left-ventricular assist device placements. Using a vibratome and a specially developed cultivation system, 300 &#181;m thick slices are placed between a fixed and a spring wire, allowing for stable and reproducible cultivation for several weeks. During cultivation, the slices are continuously stimulated according to individual settings. Contractions can be displayed and recorded in real-time, and pharmacological agents can be readily applied. User-defined stimulation protocols can be scheduled and performed to assess vital contraction parameters like post-pause-potentiation, stimulation threshold, force-frequency relation, and refractory period. Furthermore, the system enables a variable pre- and afterload setting for a more physiological cultivation.
Here, we present a step-by-step guide on how to generate a successful long-term cultivation of human left ventricular myocardial slices, using a commercial biomimetic cultivation solution.

We present a protocol for ex vivo cultivation of human ventricular myocardial tissue. It allows for detailed analysis of contraction force and kinetics, as well as the application of pre- and afterload to mimic the in vivo physiological environment more closely.

Cardiomyocyte cultivation has seen a vast number of developments, ranging from two-dimensional (2D) cell cultivation to iPSC derived organoids. In 2019, ...

High-resolution Optical Mapping of the Mouse Sino-atrial Node

Sino-atrial node (SAN) dysfunctions and associated complications constitute important causes of morbidity in patients with cardiac diseases. The development of novel pharmacological therapies to cure these patients relies on the thorough understanding of both normal physiology and pathophysiology of the SAN. Among the studies of cardiac pacemaking, the mouse SAN is widely used due to its feasibility for modifications in the expression of different genes that encode SAN ion channels or calcium handling proteins. Emerging evidence from electrophysiological and histological studies has also proved the representativeness and similarity of the mouse SAN structure and functions to larger mammals, including the presence of specialized conduction pathways from the SAN to the atrium and a complex pacemakers' hierarchy within the SAN. Recently, the technique of optical mapping has greatly facilitated the exploration and investigation of the origin of excitation and conduction within and from the mouse SAN, which in turn has extended the understanding of the SAN and benefited clinical treatments of SAN dysfunction associated diseases. In this manuscript, we have described in detail how to perform the optical mapping of the mouse SAN from the intact, Langendorff-perfused heart and from the isolated atrial preparation. This protocol is a useful tool to enhance the understanding of mouse SAN physiology and pathophysiology.

Here, we present a protocol for optical mapping of electrical activity from the mouse right atrium and especially the sino-atrial node, at a high spatial and temporal resolution.

Sino-atrial node (SAN) dysfunctions and associated complications constitute important causes of morbidity in patients with cardiac diseases. The ...

Revealing Murine Pulmonary Veins Myocardial Architecture

Microdissection and Immunofluorescence Staining of Myocardial Sleeves in Murine Pulmonary Veins

Pulmonary veins (PVs) are the major source of ectopic beats in atrial arrhythmias and play a crucial role in the development and progression of atrial fibrillation (AF). PVs contain myocardial sleeves (MS) composed of cardiomyocytes. MS are implicated in the initiation and maintenance of AF, as they preserve similarities to the cardiac working myocardium, including the ability to generate ectopic electrical impulses. Rodents are widely used and may represent excellent animal models to study the pulmonary vein myocardium since cardiomyocytes are widely present all over the vessel wall. However, precise microdissection and preparation of murine PVs is challenging due to the small organ size and intricate anatomy.
We demonstrate a microscopy-guided microdissection protocol for isolating the murine left atrium (LA) together with the PVs. Immunofluorescence staining using cardiac Troponin-T (cTNT) and connexin 43 (Cx43) antibodies is performed to visualize the LA and PVs in full length. Imaging at 10x and 40x magnification provides a comprehensive view of the PV structure as well as detailed insights into the myocardial architecture, particularly highlighting the presence of connexin 43 within the MS.

Author Spotlight: Developing a Translational Model for Atrial Fibrillation Research Across Species 

This protocol demonstrates microscopy-guided isolation and immunofluorescence staining of murine pulmonary veins. We prepare tissue samples containing the left atrium, pulmonary veins, and the corresponding lungs and stain them for cardiac Troponin T and Connexin 43.

Pulmonary veins (PVs) are the major source of ectopic beats in atrial arrhythmias and play a crucial role in the development and progression of atrial ...

Extracting Intact Kidney from Mouse: A Technique to Obtain Kidney Without Renal Capsule from Murine Models

Source: Grainger, N. et al. <a href="https://jove.unicartagenaproxy.elogim.com/video/62040" target="_blank">Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning.</a> J. Vis. Exp. (2021)
In this video, we describe the procedure for kidney extraction from the retroperitoneal space of the mouse. The extracted kidney can further be microdissected to obtain an intact kidney without a renal capsule and the surrounding fat layer.

Source: Grainger, N. et al. Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning. J. Vis. Exp. (2021)
In ...

Isolating and Imaging Live, Intact Pacemaker Regions of Mouse Renal Pelvis by Vibratome Sectioning

Summary

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Chapters in this video

Optical Imaging of Isolated Murine Ventricular Myocytes

Preclinical Cardiac Electrophysiology Assessment by Dual Voltage and Calcium Optical Mapping of Human Organotypic Cardiac Slices

Murine Short Axis Ventricular Heart Slices for Electrophysiological Studies

Mouse Fetal Whole Intestine Culture System for Ex Vivo Manipulation of Signaling Pathways and Three-dimensional Live Imaging of Villus Development

Whole-Mount Immunofluorescence Staining, Confocal Imaging and 3D Reconstruction of the Sinoatrial and Atrioventricular Node in the Mouse

Implementing Patch Clamp and Live Fluorescence Microscopy to Monitor Functional Properties of Freshly Isolated PKD Epithelium

Preparation of Human Myocardial Tissue for Long-Term Cultivation

High-resolution Optical Mapping of the Mouse Sino-atrial Node

Microdissection and Immunofluorescence Staining of Myocardial Sleeves in Murine Pulmonary Veins

Extracting Intact Kidney from Mouse: A Technique to Obtain Kidney Without Renal Capsule from Murine Models