The authors thank Christina Schwandt, Blanka Duvnjak, and Nicola Kuhr for their exceptional technical assistance and Dr. Dennis Sohn for his help with the fluorescence scan.This research was supported by a grant of the Deutsche Forschungsgemeinschaft (DFG) SFB 612 TP B18 to L.C.R. and L.S. The funder had no role in the study design, data collection and analysis, decision to publish, or preparation of the manuscript.

The investigations were conducted according to the guidelines outlined in the Guide for Care and Use of Laboratory Animals (US National Institutes of Health Publication No. 85-23, revised 1996). All animal experiments were performed in accordance with the relevant institutional approvals (state government Landesamt f&#252;r Natur, Umwelt und Verbraucherschutz [LANUV] reference number 84-02.04.2012.A397).
1. Preparation of instruments, solutions, and equipment
<ol>
	<li>Reconstitute FITC-polysucrose 70 with 0.9% sterile sodium chloride (NaCl) to a final concentration of 10 mg/mL (i.e., 100 mg in 10 mL of NaCl).</li>
	<li>Dialyze FITC-polysucrose 70 solution to remove free FITC molecules overnight at 4 &#176;C (molecular weight cut-off [MWCO] at 10,000). Use 1 L of 0.9% sterile NaCl per 10 mL of FITC-polysucrose 70 under constant stirring. Protect from light. Aliquot the dialyzed FITC-polysucrose 70 and store it at -20 &#176;C.</li>
	<li>For the FITC-polysucrose 70 bolus, add 4 &#181;L of 10 mg/mL FITC-polysucrose 70 solution to 996 &#181;L of 0.9% NaCl (the final concentration of FITC-polysucrose 70: 40 &#181;g/mL).</li>
	<li>For the equilibration infusion solution, add 20 &#181;L of a 10 mg/mL FITC-polysucrose 70 solution to 9.98 mL of 0.9% sterile NaCl yielding to a final concentration of 20 &#181;g/mL.</li>
	<li>For the experimental solution, add drugs or substances to the infusion solution (e.g., for angiotensin II [Ang II] [100 ng/kg/min] for a 25 g mouse, add 3 &#181;L of Ang II of a 1 mM solution).</li>
	<li>For the surgery, prepare one shaver, two surgical clamps, one pair of surgical scissors, two tweezers, two fine tweezers, one pair of fine scissors, and swabs. Prepare two 10 cm silk threads (4-0 to 6-0) for ligation procedures.</li>
	<li>For the placement of a central venous catheter, prepare a 10 mL syringe with a 21 G needle. Place the tip of the needle in a 30 cm-long catheter (with an inner diameter [ID] of 0.58 mm). Connect the 0.58 mm catheter to a 10 cm catheter (with an ID of 0.28 mm). Cut the tip of the smaller catheter oblique to create a sharp tip that is introduced into the jugular vein.</li>
	<li>Prepare the anesthesia (i.e., intraperitoneal anesthesia ketamine, 100 mg/kg of body weight, and xylazine, 5 mg/kg of body weight).</li>
	<li>Prepare a 22 G angiocatheter by discarding the needle and marking the catheter 1 cm from the tip. Preheat the heating pad to 37 &#176;C.</li>
	<li>Prepare a blood pressure device and change the blood-pressure-measuring membrane if necessary.</li>
</ol>
2. Preparation phase
<ol>
	<li>Urinary catheter 
	NOTE: Section 2.1 follows the protocol as described by Reis et al.7. Figure 1 and Supplemental Figure 1 show the placement of a urinary catheter in female mice.
	<ol>
		<li>Anesthetize the mouse with ketamine/xylazine (see step 1.8). Use the toe-pinch test to confirm proper anesthesia. To maintain anesthesia, repeat the anesthesia (e.g., with half the dosage) after 60 min.&#160;Proper anesthesia is confirmed if toe pinch test does not result in reflex withdrawl. 
		NOTE: Female FVB mice are used in this protocol.</li>
		<li>Position the mouse in dorsal recumbency on a 37 &#176;C heating pad. Tighten the lower abdomen and find the urethral ostium (e.g., under a microscope).</li>
		<li>Use the plastic part of the catheter of a 22 G angiocatheter and lubricate it with xylocaine gel. Introduce it carefully 3 mm into the urethral ostium while paralleling the distal urethral axis (Figure 1A).</li>
		<li>Turn the top of the angiocatheter 180&#176; by keeping the tip within the urethral ostium and maintaining the axis of the urethra (Figure 1B).</li>
		<li>Introduce the catheter 7 mm further into the mouse so that it is placed within the bladder (Figure 1C). Do not force the catheter beyond resistance. Correct the position of the catheter from the beginning if resistance is felt. Take note that if the position of the urinary catheter is correct, urine might already appear within the catheter.</li>
		<li>Place a 1.5 mL brown tube over the top of the angiocatheter to collect the urine. Apply 1 mL of 0.9% NaCl subcutaneously to enhance urine production.</li>
	</ol>
	</li>
	<li>Central venous catheter 
	<ol>
		<li>Shave the neck of the mouse and place it in recumbency with the head toward the surgeon. Hyperextend the head of the mouse with a tape.</li>
		<li>Disinfect the neck with 70% isopropanol. Make a small skin incision (5 mm) below the jawline, using a tweezer and a pair of scissors. Cut the skin approximately 1 cm in the direction of the sternum until the middle of the sternum is reached.</li>
		<li>Carefully dissect the skin on the right side of the neck, using a pair of scissors. Make a rectangular incision of the skin to the right side of the mouse to expose the soft tissue of the neck. Use a pair of scissors and a tweezer. Fix the skin flaps with two clamps. 
		NOTE: The jugular vein runs along the left side of the thyroid gland or is slightly covered by the right lobe of the thyroid gland. After this step, use a microscope for surgery.</li>
		<li>Carefully expose the jugular vein by blunt preparation, using the tip of the fine tweezer. Avoid injury to vein branches. 
		NOTE: It might be necessary to remove tissue with fine scissors. Be careful when using scissors to remove tissue as it increases the risk of bleeding.</li>
		<li>Place and close a ligature with a silk thread (4-0 to 6-0) at the distal part of the visible jugular vein (toward the head of the mouse). Put tension on the ligature by fixing the silk thread with a tape to ensure slight tension on the jugular vein. Prepare a ligature around the proximal part of the jugular vein.</li>
		<li>Fill the catheter with the equilibration infusion solution (see step 1.4) and fix the catheter with a tape so that the catheter is aligning the jugular vein. Control for bubbles to avoid air embolism.</li>
		<li>Lift the jugular vein with fine tweezers at the site of insertion (the insertion site is 1&#8211;2 mm proximal of the ligature). Align the tubing parallel to the jugular vein. Puncture the jugular vein, aiming for the lumen, and insert for approximately 2&#8211;4 mm, paralleling the axis of the jugular vein. Avoid any brisk movements.</li>
		<li>Close the ligature to fix the catheter. Control for tightness of the ligature by carefully viewing through the microscope. Put a damp swab over the site of surgery.</li>
	</ol>
	</li>
	<li>Blood pressure measurement
	<ol>
		<li>Place the tail-cuff at the bottom of the mouse tail while the mouse lays in dorsal recumbency. Start the measurements and repeat them 10x per time point. Build a mean from the measurements.</li>
		<li>Adjust the position of the tail-cuff if blood pressure measurements do not seem correct and false data are produced.</li>
	</ol>
	</li>
</ol>
3. Equilibration phase
<ol>
	<li>Change the urinary collection tube before the equilibration phase starts and place it on ice.</li>
	<li>Introduce a 10 mL syringe filled with FITC equilibration phase solution (see step 1.4) with a 21 G needle and the larger catheter (with an ID of 0.58 mm) and place it into the syringe pump.</li>
	<li>Fold a swab and put it around the small-vessel catheter (with an ID of 0.28 mm) that is introduced into the jugular vein. Lay the catheter inside the swab. Place a clamp over the swab to abolish retrograde blood flow or air embolism. Connect a 27 G needle with a 1 mL syringe filled with the FITC bolus to the end of the small-vessel catheter.</li>
	<li>Open the clamp and apply the FITC bolus (100 &#181;L). Close the clamp again and connect the larger catheter with the smaller catheter. Start the syringe pump with 0.008 mL/min (0.480 mL/h). Continue the infusion for 60 min.</li>
</ol>
4. Experimental phase
NOTE: In this phase, the effect of drugs on glomerular permselectivity can be investigated.
<ol>
	<li>Change the urinary tube (time point 0 min) to another 1.5 mL brown tube. Put a swab around the small-vessel catheter and close a clamp as indicated in step 3.3.</li>
	<li>Disconnect the large catheter from the small-vessel catheter. Change the syringes to the experimental phase solutions (see step 1.5). Let the infusion pump run so that the large catheter is filled with the equilibration solution.</li>
	<li>Reconnect the catheters while avoiding air embolism and reopen the clamp. Start the syringe pump at 0.008 mL/min.</li>
	<li>Continue running the syringe pump for 60 min and collect the urine within the urinary tube thereafter (urine 60 min). Place the urine tube on ice.</li>
	<li>Sacrifice the mouse by cervical dislocation during anesthesia. Prior to disposal the mouse is observed for 5 minutes to ensure it is dead.</li>
</ol>
5. Urine analysis
<ol>
	<li>Fluorescence measurement
	<ol>
		<li>Thaw the urinary pool and dilute it 1:10 with phosphate-buffered saline (PBS). 
		NOTE: The urinary pool is a pool of urine that has been collected from healthy mice in a 12&#8211;24 h urine collection in a metabolic cage.</li>
		<li>Prepare standards for the fluorescence measurement. Take 10 brown 1.5 mL tubes and label them for blank (1:10 diluted urine pool) and the following FITC-polysucrose 70 concentrations (0.625, 1.25, 2.5, 5, 10, 20, 40, 80, and 160 &#181;g/mL).</li>
		<li>Pipet 246 &#181;L of diluted urine pool into a 1.5 mL brown tube and add 4 &#181;L of the FITC-polysucrose 70 stock concentration (see step 1.1) to get a final concentration of 160 &#181;g/mL FITC-polysucrose 70. Pipet 100 &#181;L of the diluted urine pool into all other tubes.</li>
		<li>Dilute 1:2 by pipetting 100 &#181;L of the 160 &#181;g/mL FITC-polysucrose 70 tube into the 80 &#181;g/mL tube and continue with the other concentrations. Assure proper mixture of the diluted concentrations (e.g., by vortexing the tube before continuing).</li>
		<li>Dilute the mouse urine samples (0 min, 60 min) 1:10 with diluted urinary pool.</li>
		<li>Pipette 5 &#181;L of each standard FITC-polysucrose 70 concentration and of the mouse urine samples as triplicates in a black 384-well plate. Centrifuge the plate at 1,000 x g for 15 s to avoid bubbles.</li>
		<li>Analyze the 384-well plate in a plate reader. Perform excitation at 496 nm and measure the fluorescence at 525 nm.</li>
	</ol>
	</li>
	<li>Creatinine measurement
	<ol>
		<li>Follow the manufacturer&#8217;s instructions. In brief, prepare creatinine standards by diluting 10 &#181;L of the 100 mM creatinine standard solution with 990 &#181;L of creatinine assay buffer to prepare a 1 mM standard solution.</li>
		<li>Add 0, 2, 4, 6, 8, and 10 &#181;L of the 1 mM creatinine standard solution into a 96-well plate to generate 0, 2, 4, 6, 8, and 10 nmol/well standards, respectively. Add creatinine assay buffer to each well to bring the volume to 50 &#181;L.</li>
		<li>Prepare the reaction mixes by adding 42&#8211;44 &#181;L of creatinine assay buffer, 2 &#181;L of creatinase, 2 &#181;L of creatininase, 2 &#181;L of creatinine enzyme mix, and 2 &#181;L of creatinine probe. For the blank, use 44 &#181;L of creatinine assay buffer, 2 &#181;L of creatinase, 2 &#181;L of creatinine enzyme mix, and 1&#8211;2 &#181;L of creatinine probe.</li>
		<li>Add 50 &#181;L of the appropriate reaction mix to each well in the 96-well plate and incubate it for 60 min on a horizontal shaker at 37 &#176;C. Protect the plate from light during the incubation. Measure the absorbance at 570 nm on a plate reader.</li>
		<li>Calculate the creatinine concentrations by subtracting the blank value from all readings. The result will have the unit nanomoles/microliter. Multiply the concentration of creatinine by the molecular weight of creatinine (113.12 ng/nmol) to receive the unit nanograms/microliter.</li>
	</ol>
	</li>
</ol>
6. Data analysis
<ol>
	<li>Calculate the FITC-polysucrose 70 urine concentration from the standard curve.</li>
	<li>Reference the FITC-polysucrose 70 urine concentrations to creatinine concentrations in the representative urine sample.</li>
	<li>Reference the urine 60 min samples to urine 0 min samples of controls and treated mice.</li>
</ol>

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The authors have nothing to disclose.

The presented method enables the investigator to test glomerular permeability in mice in a very sensitive manner using a tracer. With this method, short-term increases in glomerular permeability can be diagnosed using only small amounts of urine. The most critical steps for successfully mastering this technique are 1) developing manual expertise in mouse surgery, especially in the cannulation of a central vein, 2) placing the urinary catheter without harming the mucosa, and 3) manual expertise in handling 384-well plates...

Functional or structural defects within the glomerular filtration barrier increase glomerular permeability to albumin, resulting in the detection of albumin in the urine (albuminuria). Albuminuria predicts cardiovascular outcome and is an important marker for glomerular injury1. Even low levels of albuminuria, lying within the normal range, are associated with an increased cardiovascular risk1.
Under physiological conditions, albumin is filtered through the glomerulus and is almost completely reabsorbed in the tubular system2,3. In mice, the detection of albumin in the urine is usually performed by an albumin enzyme-linked immunosorbent assay (ELISA) from 24 h of urine collection. If urine from a 24 h urine collection or spot urine is used, small differences in albumin concentrations may be missed due to assay sensitivity problems. Most researchers, therefore, use animal models in which albuminuria is induced by robust renal injury due to toxins, drugs, and renal surgery.
Therefore, the finding of a sensitive method to detect small and transient changes in glomerular permeability is very important to the field. Rippe et al. have presented a rat model to test glomerular permeability by applying a fluorescently labeled tracer, namely FITC-polysucrose 70 (i.e., FITC-Ficoll 70), at the size of albumin4. The tracer application allows the testing of short-term changes in glomerular permeability (within minutes) and is very sensitive4. Two studies have used the tracer method in mice5,6. Despite its benefits, this method, unfortunately, has disadvantages: it is technically very complex, radioactive, and invasive. Further analysis of the urine is only accomplished by using gel filtration or size-exclusion HPLC5,6.
Within this paper, we present an alternative, sensitive, nonradioactive, and fast method to measure glomerular permeability in mice using fluorescently labeled FITC-polysucrose 70. By introducing a transurethral catheter, urine collection is less invasive than bladder puncture, urethrotomy, and suprapubic catheter application, and allows urine collection at least every 30 min. Urine analysis is performed from small amounts (5&#181;L) using a fluorescent plate reader. Tracer concentrations in the urine are normalized to creatinine concentrations in the urine using an enzymatic creatinine assay.
Therefore, this novel method offers a sensitive tool to study early glomerular injury with increased glomerular permeability.

<table border="0" cellpadding="0" cellspacing="0" style="width:671px;" width="669">
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">Motic SMZ168 BL</td>
			<td style="width:77px;">Motic</td>
			<td style="width:101px;">SMZ168BL</td>
			<td style="width:235px;">microscope for mouse surgery</td>
		</tr>
		<tr height="84">
			<td height="84" style="height:84px;width:257px;">KL1500LCD</td>
			<td style="width:77px;">Pulch and Lorenz microscopy</td>
			<td style="width:101px;">150500</td>
			<td>light for mouse surgery</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Microfederschere</td>
			<td style="width:77px;">Braun, Aesculap</td>
			<td style="width:101px;">FD100R</td>
			<td>fine scissors</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Durotip Feine Scheren</td>
			<td style="width:77px;">Braun, Aesculap</td>
			<td style="width:101px;">BC210R</td>
			<td>for neck cut</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Anatomische Pinzette</td>
			<td style="width:77px;">Braun, Aesculap</td>
			<td style="width:101px;">BD215R</td>
			<td>for surgery&#160;</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">Pr&#228;parierklemme</td>
			<td style="width:77px;">Aesculap</td>
			<td style="width:101px;">BJ008R</td>
			<td>for surgery&#160;</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Seraflex</td>
			<td style="width:77px;">Serag Wiessner</td>
			<td style="width:101px;">IC108000</td>
			<td>silk thread</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">Ketamine 10%</td>
			<td style="width:77px;">Medistar</td>
			<td style="width:101px;"></td>
			<td>anesthesia</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">Rompun (Xylazin) 2%</td>
			<td style="width:77px;">Bayer</td>
			<td style="width:101px;"></td>
			<td>anesthesia</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Fine Bore Polythene Tubing ID 0.28mm OD 0.61mm</td>
			<td style="width:77px;">Portex</td>
			<td style="width:101px;">800/100/100</td>
			<td style="width:235px;">Catheter</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Fine Bore Polythene Tubing ID 0.58mm OD 0.96mm</td>
			<td style="width:77px;">Portex</td>
			<td style="width:101px;">800/100/200</td>
			<td style="width:235px;">Catheter</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Harvard apparatus 11 Plus</td>
			<td style="width:77px;">Harvard Apparatus</td>
			<td style="width:101px;">70-2209</td>
			<td>syringe pump</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;"></td>
			<td style="width:77px;"></td>
			<td style="width:101px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">BD Insyte Autoguard</td>
			<td style="width:77px;">BD</td>
			<td style="width:101px;">381823</td>
			<td>&#160;urinary catheter</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Multimode Detector DTX 880</td>
			<td style="width:77px;">Beckman Coulter</td>
			<td style="width:101px;"></td>
			<td>plate reader</td>
		</tr>
		<tr height="25">
			<td height="25" style="height:25px;width:257px;">384 well microtiterplate</td>
			<td style="width:77px;">Nunc</td>
			<td style="width:101px;">262260</td>
			<td style="width:235px;">384 well platte</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Creatinine Assay Kit</td>
			<td style="width:77px;">Sigma-Aldrich</td>
			<td style="width:101px;">MAK080</td>
			<td>to measure creatinine concentration</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">96 well plate</td>
			<td style="width:77px;">Nunc</td>
			<td style="width:101px;">260836</td>
			<td>for creatinine assay&#160;</td>
		</tr>
		<tr height="63">
			<td height="63" style="height:63px;width:257px;">FITC-labeled polysuccrose 70</td>
			<td style="width:77px;">TBD Consultancy</td>
			<td style="width:101px;">FP70</td>
			<td>FITC-ficoll</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:257px;">Angiotensin II</td>
			<td style="width:77px;">Sigma-Aldrich</td>
			<td style="width:101px;">A9525</td>
			<td>used to test glomerular permeability</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">BP-98A</td>
			<td style="width:77px;">Softron</td>
			<td style="width:101px;"></td>
			<td>for blood pressure measurement</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">OTS 40.3040</td>
			<td style="width:77px;">Medite</td>
			<td style="width:101px;">01-4005-00</td>
			<td>heating plate for mouse surgery</td>
		</tr>
		<tr height="63">
			<td height="63" style="height:63px;width:257px;">Instillagel 6mL</td>
			<td style="width:77px;">Farco-Pharma GmbH</td>
			<td style="width:101px;"></td>
			<td>for urinary catheter</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:257px;">Exacta</td>
			<td style="width:77px;">Aesculap</td>
			<td style="width:101px;">GT415</td>
			<td>shaver</td>
		</tr>
	</tbody>
</table>

highly sensitive measurement of glomerular permeability in mice with fluorescein isothiocyanate-polysucrose 70

The loss of albumin in urine (albuminuria) predicts cardiovascular outcome. Under physiological conditions, small amounts of albumin are filtered by the glomerulus and reabsorbed in the tubular system up until the absorption limit is reached. Early increases in pathological albumin filtration may, thus, be missed by analyzing albuminuria. Therefore, the use of tracers to test glomerular permselectivity appears advantageous. Fluorescently labeled tracer fluorescein isothiocyanate (FITC)-polysucrose (i.e., FITC-Ficoll), can be used to study glomerular permselectivity. FITC-polysucrose molecules are freely filtered by the glomerulus but not reabsorbed in the tubular system. In mice and rats, FITC-polysucrose has been investigated in models of glomerular permeability by using technically complex procedures (i.e., radioactive measurements, high-performance liquid chromatography [HPLC], gel filtration). We have modified and facilitated a FITC-polysucrose tracer-based protocol to test early and small increases in glomerular permeability to FITC-polysucrose 70 (size of albumin) in mice. This method allows repetitive urine analyses with small urine volumes (5 &#181;L). This protocol contains information on how the tracer FITC-polysucrose 70 is applied intravenously and urine is collected via a simple urinary catheter. Urine is analyzed via a fluorescence plate reader and normalized to a urine concentration marker (creatinine), thereby avoiding technically complex procedures.

As depicted in Figure 2, the method to test glomerular permeability in mice is built up in three phases. The first phase is called the preparation phase, in which a urinary catheter and a central venous catheter are placed. The second phase is called the equilibration phase, starting with an intravenous bolus injection of FITC-polysucrose 70 and followed by the continuous infusion of FITC-polysucrose 70 for 60 min. The last phase is called the experimental ph...

Watch this Scientific Journal Video about Highly Sensitive Measurement of Glomerular Permeability in Mice with Fluorescein Isothiocyanate-polysucrose 70 at JoVE.com

Highly Sensitive Measurement of Glomerular Permeability in Mice with Fluorescein Isothiocyanate-polysucrose 70

Here, we present a protocol to test glomerular permeability in mice using a highly sensitive, nonradioactive tracer. This method allows repetitive urine analyses with small urine volumes.

The loss of albumin in urine (albuminuria) predicts cardiovascular outcome. Under physiological conditions, small amounts of albumin are filtered by the ...

highly-sensitive-measurement-glomerular-permeability-mice-with

Universidad de Cartagena UDEC

Research

JoVE Journal

Medicine

6.8K Views.  Heinrich-Heine-University. Here, we present a protocol to test glomerular permeability in mice using a highly sensitive, nonradioactive tracer. This method allows repetitive urine analyses with small urine volumes.

Video: Highly Sensitive Measurement of Glomerular Permeability in Mice with Fluorescein Isothiocyanate-polysucrose 70

Identification and Isolation of Slow-Dividing Cells in Human Glioblastoma Using Carboxy Fluorescein Succinimidyl Ester (CFSE)

Tumor heterogeneity represents a fundamental feature supporting tumor robustness and presents a central obstacle to the development of therapeutic strategies1. To overcome the issue of tumor heterogeneity, it is essential to develop assays and tools enabling phenotypic, (epi)genetic and functional identification and characterization of tumor subpopulations that drive specific disease pathologies and represent clinically relevant targets. It is now well established that tumors exhibit distinct sub-fractions of cells with different frequencies of cell division, and that the functional criteria of being slow cycling is positively associated with tumor formation ability in several cancers including those of the brain, breast, skin and pancreas as well as leukemia2-8. The fluorescent dye carboxyfluorescein succinimidyl ester (CFSE) has been used for tracking the division frequency of cells in vitro and in vivo in blood-borne tumors and solid tumors such as glioblastoma2,7,8. The cell-permeant non-fluorescent pro-drug of CFSE is converted by intracellular esterases into a fluorescent compound, which is retained within cells by covalently binding to proteins through reaction of its succinimidyl moiety with intracellular amine groups to form stable amide bonds9. The fluorescent dye is equally distributed between daughter cells upon divisions, leading to the halving of the fluorescence intensity with every cell division. This enables tracking of cell cycle frequency up to eight to ten rounds of division10. CFSE retention capacity was used with brain tumor cells to identify and isolate a slow cycling subpopulation (top 5% dye-retaining cells) demonstrated to be enriched in cancer stem cell activity2. 
This protocol describes the technique of staining cells with CFSE and the isolation of individual populations within a culture of human glioblastoma (GBM)-derived cells possessing differing division rates using flow cytometry2. The technique has served to identify and isolate a brain tumor slow-cycling population of cells by virtue of their ability to retain the CFSE labeling.

Identification and Isolation of Slow-Dividing Cells in Human Glioblastoma Using Carboxy Fluorescein Succinimidyl Ester CFSE

This video protocol demonstrates the application of the fluorescent dye carboxyfluorescein succinimidyl ester (CFSE) for the identification and separation of different sub-populations of cells in human glioblastoma based on frequency of cell division.

Tumor heterogeneity represents a fundamental feature supporting tumor robustness and presents a central obstacle to the development of therapeutic ...

Quantifying Glomerular Permeability of Fluorescent Macromolecules Using 2-Photon Microscopy in Munich Wistar Rats

Kidney diseases involving urinary loss of large essential macromolecules, such as serum albumin, have long been thought to be caused by alterations in the permeability barrier comprised of podocytes, vascular endothelial cells, and a basement membrane working in unison. Data from our laboratory using intravital 2-photon microscopy revealed a more permeable glomerular filtration barrier (GFB) than previously thought under physiologic conditions, with retrieval of filtered albumin occurring in an early subset of cells called proximal tubule cells (PTC)1,2,3.
Previous techniques used to study renal filtration and establishing the characteristic of the filtration barrier involved micropuncture of the lumen of these early tubular segments with sampling of the fluid content and analysis4. These studies determined albumin concentration in the luminal fluid to be virtually non-existent; corresponding closely to what is normally detected in the urine. However, characterization of dextran polymers with defined sizes by this technique revealed those of a size similar to serum albumin had higher levels in the tubular lumen and urine; suggesting increased permeability5.
Herein is a detailed outline of the technique used to directly visualize and quantify glomerular fluorescent albumin permeability in vivo. This method allows for detection of filtered albumin across the filtration barrier into Bowman's space (the initial chamber of urinary filtration); and also allows quantification of albumin reabsorption by proximal tubules and visualization of subsequent albumin transcytosis6. The absence of fluorescent albumin along later tubular segments en route to the bladder highlights the efficiency of the retrieval pathway in the earlier proximal tubule segments. Moreover, when this technique was applied to determine permeability of dextrans having a similar size to albumin virtually identical permeability values were reported2. These observations directly support the need to expand the focus of many proteinuric renal diseases to included alterations in proximal tubule cell reclamation.

A technique utilizing high resolution intavital 2-photon microscopy to directly visualize and quantify gloemrular filtration in surface glomeruli. This method allows for direct determination of permeability characteristics of macromolecules in both normal and diseased states.

Kidney  diseases involving urinary loss of large essential macromolecules, such as  serum albumin, have long been thought to be caused by alterations in ...

An in vivo Assay to Test Blood Vessel Permeability

This method is based on the intravenous injection of Evans Blue in mice as the test animal model. Evans blue is a dye that binds albumin. Under physiologic conditions the endothelium is impermeable to albumin, so Evans blue bound albumin remains restricted within blood vessels. In pathologic conditions that promote increased vascular permeability endothelial cells partially lose their close contacts and the endothelium becomes permeable to small proteins such as albumin. This condition allows for extravasation of Evans Blue in tissues. A healthy endothelium prevents extravasation of the dye in the neighboring vascularized tissues. Organs with increased permeability will show significantly increased blue coloration compared to organs with intact endothelium. The level of vascular permeability can be assessed by simple visualization or by quantitative measurement of the dye incorporated per milligram of tissue of control versus experimental animal/tissue. Two powerful aspects of this assay are its simplicity and quantitative characteristics. Evans Blue dye can be extracted from tissues by incubating a specific amount of tissue in formamide. Evans Blue absorbance maximum is at 620 nm and absorbance minimum is at 740 nm. By using a standard curve for Evans Blue, optical density measurements can be converted into milligram dye captured per milligram of tissue. Statistical analysis should be used to assess significant differences in vascular permeability.

An in vivo Assay to Test Blood Vessel Permeability

We are presenting an in vivo assay to test blood vessel permeability. This assay is based on intravenous injection of a dye and subsequent visualization of its diffusion into interstitial spaces.

This method is based on the intravenous injection of Evans Blue in mice as the test animal model. Evans blue is a dye that binds albumin. Under ...

Carotid Artery Infusions for Pharmacokinetic and Pharmacodynamic Analysis of Taxanes in Mice

When proposing the use of a drug, drug combination, or drug delivery into a novel system, one must assess the pharmacokinetics of the drug in the study model. As the use of mouse models are often a vital step in preclinical drug discovery and drug development1-8, it is necessary to design a system to introduce drugs into mice in a uniform, reproducible manner. Ideally, the system should permit the collection of blood samples at regular intervals over a set time course. The ability to measure drug concentrations by mass-spectrometry, has allowed investigators to follow the changes in plasma drug levels over time in individual mice1, 9, 10. In this study, paclitaxel was introduced into transgenic mice as a continuous arterial infusion over three hours, while blood samples were simultaneously taken by retro-orbital bleeds at set time points. Carotid artery infusions are a potential alternative to jugular vein infusions, when factors such as mammary tumors or other obstructions make jugular infusions impractical. Using this technique, paclitaxel concentrations in plasma and tissue achieved similar levels as compared to jugular infusion. In this tutorial, we will demonstrate how to successfully catheterize the carotid artery by preparing an optimized catheter for the individual mouse model, then show how to insert and secure the catheter into the mouse carotid artery, thread the end of the catheter out through the back of the mouse&#8217;s neck, and hook the mouse to a pump to deliver a controlled rate of drug influx. Multiple low volume retro-orbital bleeds allow for analysis of plasma drug concentrations over time.

This method was developed with the goal of delivering a steady drug solution via the carotid artery, to assess the pharmacokinetics of novel drugs in mouse models.

When proposing the use of a drug, drug combination, or drug delivery into a novel system, one must assess the pharmacokinetics of the drug in the study ...

Automated Measurement of Pulmonary Emphysema and Small Airway Remodeling in Cigarette Smoke-exposed Mice

COPD is projected to be the third most common cause of mortality world-wide by 2020(1). Animal models of COPD are used to identify molecules that contribute to the disease process and to test the efficacy of novel therapies for COPD. Researchers use a number of models of COPD employing different species including rodents, guinea-pigs, rabbits, and dogs(2). However, the most widely-used model is that in which mice are exposed to cigarette smoke. Mice are an especially useful species in which to model COPD because their genome can readily be manipulated to generate animals that are either deficient in, or over-express individual proteins. Studies of gene-targeted mice that have been exposed to cigarette smoke have provided valuable information about the contributions of individual molecules to different lung pathologies in COPD(3-5). Most studies have focused on pathways involved in emphysema development which contributes to the airflow obstruction that is characteristic of COPD. However, small airway fibrosis also contributes significantly to airflow obstruction in human COPD patients(6), but much less is known about the pathogenesis of this lesion in smoke-exposed animals. To address this knowledge gap, this protocol quantifies both emphysema development and small airway fibrosis in smoke-exposed mice. This protocol exposes mice to CS using a whole-body exposure technique, then measures respiratory mechanics in the mice, inflates the lungs of mice to a standard pressure, and fixes the lungs in formalin. The researcher then stains the lung sections with either Gill&#8217;s stain to measure the mean alveolar chord length (as a readout of emphysema severity) or Masson&#8217;s trichrome stain to measure deposition of extracellular matrix (ECM) proteins around small airways (as a readout of small airway fibrosis). Studies of the effects of molecular pathways on both of these lung pathologies will lead to a better understanding of the pathogenesis of COPD.

The goal of this protocol is to provide automated methods to quantify chronic lung pathologies in a murine model of COPD. The protocol includes exposing mice to cigarette smoke (CS), measuring pulmonary function, inflating the lungs, and using morphometry methods to measure emphysema and small airway remodeling in mice.

COPD is projected to be the third most common cause of mortality world-wide by 2020(1).  Animal models of COPD are used to identify molecules that ...

Surgical Models of Gastroesophageal Reflux with Mice

Multiple surgical procedures have been reported to induce gastroesophageal reflux in animals. Herein, we report three surgical models with mice aiming to induce reflux of gastric contents, duodenal contents or mixed contents. Surgical procedures and general principles have been described in detail. A researcher with surgical experience should be able to grasp the technique after a short period of practice. After surgery, most mice can survive and develop reflux esophagitis similar to that in humans. However, it should be noted that histological differences between mouse and human esophagus are the inherent limitations of these surgical models. If used for research on Barrett&#8217;s esophagus and adenocarcinoma, these procedures may need to be combined with genetic modifications.

This article demonstrates surgical procedures of gastroesophageal reflux with mice. These models are useful tools for research on mechanisms and treatment of gastroesophageal reflux disease and potentially Barrett&#8217;s esophagus and esophageal adenocarcinoma.

Multiple surgical procedures have been reported to induce gastroesophageal reflux in animals. Herein, we report three surgical models with mice aiming to ...

Visualization of Vascular and Parenchymal Regeneration after 70% Partial Hepatectomy in Normal Mice

A modified silicone injection procedure was used for visualization of the hepatic vascular tree. This procedure consisted of in-vivo injection of the silicone compound, via a 26 G catheter, into the portal or hepatic vein. After silicone injection, organs were explanted and prepared for ex-vivo micro-CT (&#181;CT) scanning. The silicone injection procedure is technically challenging. Achieving a successful outcome requires extensive microsurgical experience from the surgeon. One of the challenges of this procedure involves determining the adequate perfusion rate for the silicone compound. The perfusion rate for the silicone compound needs to be defined based on the hemodynamic of the vascular system of interest. Inappropriate perfusion rate can lead to an incomplete perfusion, artificial dilation and rupturing of vascular trees.
The 3D reconstruction of the vascular system was based on CT scans and was achieved using preclinical software such as HepaVision. The quality of the reconstructed vascular tree was directly related to the quality of silicone perfusion. Subsequently computed vascular parameters indicative of vascular growth, such as total vascular volume, were calculated based on the vascular reconstructions. Contrasting the vascular tree with silicone allowed for subsequent histological work-up of the specimen after &#181;CT scanning. The specimen can be subjected to serial sectioning, histological analysis and whole slide scanning, and thereafter to 3D reconstruction of the vascular trees based on histological images. This is the prerequisite for the detection of molecular events and their distribution with respect to the vascular tree. This modified silicone injection procedure can also be used to visualize and reconstruct the vascular systems of other organs. This technique has the potential to be extensively applied to studies concerning vascular anatomy and growth in various animal and disease models.

Tools used for visualizing vascular regeneration require methods for contrasting the vascular trees. This film demonstrated a delicate injection technique used to achieve optimal contrasting of the vascular trees and illustrate the potential benefits resulting from a detailed analysis of the resulting specimen using &#181;CT and histological serial sections.

A modified silicone injection procedure was used for visualization of the hepatic vascular tree. This procedure consisted of in-vivo injection of the ...

Long-term Blood Pressure Measurement in Freely Moving Mice Using Telemetry

During the development of new vasoactive agents, arterial blood pressure monitoring is crucial for evaluating the efficacy of the new proposed drugs. Indeed, research focusing on the discovery of new potential therapeutic targets using genetically altered mice requires a reliable, long-term assessment of the systemic arterial pressure variation. Currently, the gold standard for obtaining long-term measurements of blood pressure in ambulatory mice uses implantable radio-transmitters, which require&#160;artery cannulation. This technique eliminates the need for tethering, restraining, or anesthetizing the animals which introduce stress and artifacts during data sampling. However, arterial blood pressure monitoring in mice via catheterization can be rather challenging due to the small size of the arteries. Here we present a step-by-step guide to illustrate the crucial key passages for a successful subcutaneous implantation of radio-transmitters and carotid artery cannulation in mice. We also include examples of long-term blood pressure activity taken from freely moving mice after a period of post-surgery recovery. Following this procedure will allow reliable direct blood pressure recordings from multiple animals simultaneously.

The goal of this protocol is to assess systemic blood pressure in conscious freely moving mice using implantable radio-telemetry devices.

During the development of new vasoactive agents, arterial blood pressure monitoring is crucial for evaluating the efficacy of the new proposed drugs. ...

Re-Arterialized Rat Partial Liver Transplantation with an in vivo Vessel-Oriented 70% Hepatectomy

Split liver transplantation and living liver donor liver transplantation were developed in the clinic to utilize liver organs in a more efficient manner. To better understand the mechanism behind these surgical procedures, a rat partial liver transplantation (PLTx) model was established for relevant surgical studies. Because of the complexity of the rat PLTx model, a protocol with detailed descriptions is required. An article published previously reported a protocol in which ex vivo hepatectomy was used to achieve 50% rat PLTx. In contrast to this protocol, we introduced a re-arterialized PLTx with an in vivo 70% hepatectomy. An updated vessel-oriented hepatectomy was incorporated into the rat PLTx to refine the microsurgical procedure. The portal veins and hepatic arteries of the left lateral lobe and the median lobe were individually dissected and ligated before removal of the liver parenchyma, thereby decreasing the probability of bleeding in the remnant liver stump. Furthermore, an end-to-side vessel anastomosis between the common hepatic artery and the enlarged proper hepatic artery was introduced to re-arterialize the hepatic artery. By using this end-to-side vessel anastomosis technique, the diameter of the anastomosis was enlarged, thereby decreasing the difficulty of hand suture and maintaining a high rate of anastomotic patency. Moreover, the cuff anastomosis of the infrahepatic vena cava was slightly modified. A section of circumferential liver parenchyma around the vena cava of a recipient was preserved during cuff anastomosis to maintain the three-dimensional shape of the vascular lumen. This section of liver parenchyma was removed after completing the anastomosis. With this modification, the step involving placement of stay sutures was omitted, thereby further shortening the cuff anastomosis time. By using this protocol of rat PLTx, a low liver enzyme level, an intact liver lobular architecture and a high survival rate were achieved after microsurgery.

Re-Arterialized Rat Partial Liver Transplantation with an in vivo Vessel-Oriented 70% Hepatectomy

Here, a protocol involving re-arterialized rat partial liver transplantation is presented. Specifically, 70% liver was resected in vivo by using an updated technique of vessel-oriented hepatectomy. The hepatic artery was reconstructed in an end-to-side manner. The cuff technique was modified to shorten the anastomosis time of the infrahepatic vena cava.

Split liver transplantation and living liver donor liver transplantation were developed in the clinic to utilize liver organs in a more efficient manner. ...

Assessment of Kidney Function in Mouse Models of Glomerular Disease

The use of murine models to mimic human kidney disease is becoming increasingly common. Our research is focused on the assessment of glomerular function in diabetic nephropathy and podocyte-specific VEGF-A knock-out mice; therefore, this protocol describes the full kidney work-up used in our lab to assess these mouse models of glomerular disease, enabling a vast amount of information regarding kidney and glomerular function to be obtained from a single mouse. In comparison to alternative methods presented in the literature to assess glomerular function, the use of the method outlined in this paper enables the glomerular phenotype to be fully evaluated from multiple aspects. By using this method, the researcher can determine the kidney phenotype of the model and assess the mechanism as to why the phenotype develops. This vital information on the mechanism of disease is required when examining potential therapeutic avenues in these models. The methods allow for detailed functional assessment of the glomerular filtration barrier through measurement of the urinary albumin creatinine ratio and individual glomerular water permeability, as well as both structural and ultra-structural examination using the Periodic Acid Schiff stain and electron microscopy. Furthermore, analysis of the genes dysregulated at the mRNA and protein level enables mechanistic analysis of glomerular function. This protocol outlines the generic but adaptable methods that can be applied to all mouse models of glomerular disease.

This protocol describes a full kidney work-up that should be carried out in mouse models of glomerular disease. The methods allow for detailed functional, structural, and mechanistic analysis of glomerular function, which can be applied to all mouse models of glomerular disease.

The use of murine models to mimic human kidney disease is becoming increasingly common. Our research is focused on the assessment of glomerular function ...

Highly Sensitive Measurement of Glomerular Permeability in Mice with Fluorescein Isothiocyanate-polysucrose 70

Summary

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Chapters in this video

Identification and Isolation of Slow-Dividing Cells in Human Glioblastoma Using Carboxy Fluorescein Succinimidyl Ester (CFSE)

Quantifying Glomerular Permeability of Fluorescent Macromolecules Using 2-Photon Microscopy in Munich Wistar Rats

An in vivo Assay to Test Blood Vessel Permeability

Carotid Artery Infusions for Pharmacokinetic and Pharmacodynamic Analysis of Taxanes in Mice

Automated Measurement of Pulmonary Emphysema and Small Airway Remodeling in Cigarette Smoke-exposed Mice

Surgical Models of Gastroesophageal Reflux with Mice

Visualization of Vascular and Parenchymal Regeneration after 70% Partial Hepatectomy in Normal Mice

Long-term Blood Pressure Measurement in Freely Moving Mice Using Telemetry

Re-Arterialized Rat Partial Liver Transplantation with an in vivo Vessel-Oriented 70% Hepatectomy

Assessment of Kidney Function in Mouse Models of Glomerular Disease