Name: non-invasive assessment of the efficacy of new therapeutics for intestinal pathologies using serial endoscopic imaging of live mice
Uploaded: 2015-03-10T13:00:00
Duration: 9 min 1 s
Description: Watch this Scientific Journal Video about Non-invasive Assessment of the Efficacy of New Therapeutics for Intestinal Pathologies Using Serial Endoscopic Imaging of Live Mice at JoVE.com

We would like to thank CSL Ltd. for supporting the purchase of the endoscopy equipment. The research in the laboratory of ME is supported by the Ludwig Institute for Cancer Research, and the laboratories of TP and ME are supported by the Victorian State Government Operational Infrastructure Support and the National Health and Medical Research Council of Australia. ME is an NHMRC Senior Research Fellow.

The Walter and Eliza Hall Institute of Medical Research animal ethics committee approved each of the procedures described in these protocols.
1. Preparation of Experimental Mice
<ol>
	<li>Compose experimental cohorts of at least 4 gender matched 6-8 week old C57BL/6 mice (M. musculus) that are bred and housed in the same specific pathogen free (SPF) animal facility/room and provided with autoclaved food and water. The use of female mice will permit co-housing of mice from different lines, limit box numbers, and reduce cage-to-cage variation.</li>
	<li>Ensure that mice are at least 6 weeks of age to enable endoscopy procedures using the 3.0 mm diameter endoscopy sheath.</li>
	<li>Use mice of the same genetic background, and where possible, from cages stored on the same rack to reduce variations associated with the intestinal microflora. Variations in microflora between animal facilities should be taken into consideration when determining the appropriate control mice and genotypes for each experiment22.</li>
	<li>Mark mice by ear/toe clippings, tattoos, or similar to allow for easy identification.</li>
	<li>Weigh mice on Day 0, to determine baseline experimental weights.</li>
	<li>Perform endoscopy (see Section 5) of mice on Day 0 to record baseline colonic phenotypes.</li>
</ol>
2. Pre-clinical Trial in an Epithelial Damage and Acute Colitis Model
<ol>
	<li>Prepare a solution of the therapeutic agent to be tested. For therapeutics delivered by oral gavage (p.o.), prepare solutions to a maximum volume of 100 &#181;l. For therapeutics delivered by intraperitoneal (i.p.) injection, prepare solutions to a maximum volume of 200 &#181;l. 
	NOTE: Repeated i.p. or p.o. drug administration over prolonged periods of time can result in altered mouse behavior. Alternate the i.p. injection site to avoid prolonged discomfort. For p.o. administration, provide the mice with autoclaved sunflower seeds as a &#8216;treat&#8217; to minimize the adverse association with the gavage procedure.</li>
	<li>On Day 1, administer the therapeutic of interest (prepared in step 2.1) and appropriate vehicle controls. In the example provided (Figure 6A), 5 &#181;g of recombinant human (rh) iInterleukin (IL)-11 protein was dissolved in 200 &#181;l phosphate buffered saline (PBS) and administered i.p.</li>
	<li>Determine the timing and frequency of the administrations, which will be dependent on the pharmacokinetic profile established for the therapeutic reagent that is being tested. Figure 1 outlines prophylactic treatment using twice daily i.p. injections over the course of the experiment.</li>
	<li>Monitor, including stool consistency and the presence of blood, and weigh each mouse daily. On the days of treatment, weighing should coincide with administration of the therapeutic drug to minimize stress to the mice caused by repeated handling.</li>
	<li>On Day 3, prepare 2.5% (2.5 g/100 ml) DSS solution in the drinking water routinely provided to the mice by the animal facility. Approximately 5 ml/mouse/day of DSS solution is required for the experiment. The consumption of the DSS water may change if the ambient temperature of the animal facility fluctuates. 
	NOTE: DSS is an irritant and should be handled in accordance with MSDS instructions.</li>
	<li>Provide fresh DSS to the mice ad libitum in clean water bottles for 5 continuous days. On the evening of Day 5, provide normal drinking water in addition to mashed food pellets and a protein supplement provided in small petri dishes (100 g food pellets/10 g protein shake/10 ml water). This prevents dehydration and assists with minimizing severe weight-loss.</li>
	<li>Euthanize mice by CO2 intoxication and collect tissues for subsequent histological analysis on the morning of Day 8, or when the mice experience &#8805;15% weight-loss for more than three consecutive days, whichever occurs first. 
	NOTE: Adjust the DSS dose between 1-4% (w/v) depending on the microflora of the animal facility and the batch of DSS. Carry out, routine batch testing to establish the appropriate DSS dosage and circumvent batch-to-batch variation. The appropriate dosage should be based on weight-loss (not greater than 15% of original weight) and confirmed colitis histopathology.</li>
</ol>
3. Pre-clinical Trial in a Chronic Colitis or Colitis-associated Cancer Model
<ol>
	<li>For the chronic colitis model begin from step 3.7.</li>
	<li>For the colitis-associated cancer (CAC) model, on Day 1, inject each mouse with 10 mg/kg (w/w) Azoxymethane (AOM, 250 &#181;l, i.p.). 
	NOTE: AOM is a carcinogen and should be handled in accordance with MSDS instructions.</li>
	<li>Stock solutions of AOM are prepared as 10 mg/ml aliquots and stored at -20 &#176;C. On the day of injection, the AOM stock solution is thawed and diluted to 1 mg/ml in PBS. Repeated freezing and thawing of the AOM stock solution should be avoided.</li>
	<li>The AOM dose may be adjusted between 8-12 mg/kg. Routine batch testing is required to establish the appropriate AOM dosage in order to circumvent toxicity to mice due to batch-to-batch variation.</li>
	<li>During Days 1-7 following AOM administration weights will be stable and for this reason weight monitoring can be omitted during Days 1-7 to avoid handling animals that will excrete cytotoxic metabolites in their feces.</li>
	<li>On Day 7 all bedding needs to be changed following cytotoxic procedures. Once the bedding change is complete, the animals no longer require cytotoxic handling procedures, as they will no longer be excreting cytotoxic metabolites.</li>
	<li>On Day 8, prepare 2.5% (2.5 g/100 ml) DSS solution (as described in step 2.5) and provide to the mice ad libitum.</li>
	<li>Weigh mice daily throughout the experiment and monitor for signs of illness, including ruffled fur, hunching, bloody stools and reduced movement.</li>
	<li>On Day 13, remove the DSS solution and provide the mice with normal drinking water until Day 28. Days 8-28 constitute one &#8216;cycle&#8217; of the chronic colitis/CAC protocol.</li>
	<li>On Days 13-28, when the mice are given normal drinking water, provide the mice with mashed food pellets and a protein supplement provided in small petri dishes (100 g food pellets/10 g protein shake/10 ml water). This prevents dehydration and assists with minimizing severe weight-loss. 
	NOTE: The protein supplements in mash should not be provided when the mice are receiving DSS-containing drinking water in order to ensure consistency in DSS consumption.</li>
	<li>On Day 20 perform the second endoscopic examination to monitor individual mouse health (see Section 5).</li>
	<li>On Day 29 repeat the DSS cycle (Cycle 2: 2.5% (w/v) DSS provided during Days 29-33 and normal drinking water during Days 34-50).</li>
	<li>On Day 40 perform the third endoscopic examination to monitor individual mouse health and determine tumor burden (see Section 5).</li>
	<li>If no tumors are visible by endoscopy on Day 40, begin a third DSS cycle on Days 50-72 (Cycle 3: 2.5% (w/v) DSS provided during Days 50-55 and normal drinking water during Days 56-72). Generally, tumors are visible by Day 40 and therefore the third cycle of DSS can be omitted.</li>
	<li>Once tumors become visible by endoscopic examination, assign each mouse an endoscopic tumor score (see Section 5) and assign individual mice to cohorts with similar baseline tumor burdens.</li>
	<li>On Day 42 (or when tumors are visible), administer the therapeutic compound or relevant vehicle control (See Section 2.2). The timing of the doses will be dependent on the pharmacokinetic profile of the therapeutic. An example of an intervention treatment injected i.p. three times weekly in mice with established tumors is provided (Figure 2).</li>
	<li>Perform endoscopic exams once per week over the duration of the therapeutic treatment to monitor tumor burden. Generally, 4 weeks of a therapeutic treatment is sufficient to observe an objective treatment response. Following cessation of the treatment, a cohort of mice can also be monitored by endoscopy for tumor relapse.</li>
	<li>Euthanize mice by CO2 intoxication and collect tissues for biochemical and/or histological analysis on the morning of Day 72 or when mice experience &#8805;15% weight-loss for more than three consecutive days, whichever occurs first.</li>
</ol>
4. Pre-clinical Trial in a Sporadic Colorectal Cancer Model
<ol>
	<li>On Day 1, inject each mouse i.p. with 10 mg/kg AOM (see step 3.2). The AOM dose may be adjusted between 8-12 mg/kg. Routine batch testing is required to establish the appropriate AOM dosage in order to circumvent toxicity to mice due to batch-to-batch variation.</li>
	<li>Repeat the injection on the first day of each week for the following 5 weeks (Figure 3). The mice should be handled according to cytotoxic safety procedures for the entire 6 weeks.</li>
	<li>Weigh each mouse on the day of AOM injection to minimize distress to the mice caused by repeated handling. 
	NOTE: AOM is a carcinogen and should be handled in accordance with MSDS instructions.</li>
	<li>All animals should be handled according to cytotoxic safety procedures for the 6 weeks of AOM i.p. injections required for this protocol.</li>
	<li>During week 8 perform endoscopic examination to monitor for emerging tumors (see Section 5). Endoscopic examination should be performed every two weeks until tumors become visible. Generally, wild-type C57Bl/6 animals begin to develop tumors by approximately 40 weeks after the initial administration of AOM.</li>
	<li>Once tumors become visible by endoscopic examination, assign each mouse an endoscopic tumor score (see Section 5) and assign individual mice to a cohort with similar tumor burdens prior to the commencement of therapeutic treatment.</li>
	<li>During week 40 (or when tumors are first visible), administer the therapeutic compound or the relevant vehicle control.</li>
	<li>The timing of the doses will be dependent on the pharmacokinetic profile of the therapeutic (see step 2.1). An example of an intervention treatment injected i.p. 3 times weekly in mice with established tumors is provided (Figure 3).</li>
	<li>Perform endoscopic examination weekly for the duration of the therapeutic treatment periods to monitor tumor burden. Generally, 4 weeks of a therapeutic treatment is sufficient for an objective treatment response. Following treatment cessation, a cohort of mice can also be monitored by endoscopy for tumor relapse.</li>
	<li>Euthanize mice by CO2 intoxication and collect tissues for biochemical and/or histological analysis of the colon and tumors during week 45, or following 4 weeks of therapy.</li>
</ol>
5. Endoscopic Examinations
<ol>
	<li>The endoscopy equipment should be assembled according to standard procedures16.</li>
	<li>Sterilize and clean the endoscope probe with 70% ethanol or an anti-bacterial lubricant.</li>
	<li>Videos can be recorded using a laptop or desktop computer and standard media software, such as iMovie. A standard computer monitor, rather than a medical grade monitor, is sufficient to visualize the colon during the endoscopy procedure (Figure 4).</li>
	<li>Anesthetize groups of 5-6 mice simultaneously in a chamber with 3% isoflurane in 100% O2 at a rate of 0.2-0.4 L/min. Once the mice are anesthetized, which is confirmed by toe pinch; the isoflurane levels should be altered to 0.5-2% for maintenance.</li>
	<li>Remove an individual mouse from the chamber, and place it ventral side up with its head secured in a nose-cone. Full anesthesia should be monitored and the hind legs should be adjusted so that they are stretched out behind the mouse.</li>
	<li>Place a vet ointment on the eyes of the mice to prevent dryness.</li>
	<li>Hold the tail of the mouse where it meets the lower spine to clearly reveal the anus. Insert the rigid endoscope sheath into a beaker of water and adjust the airflow to allow the release of one small bubble at a time.</li>
	<li>The airflow will permit the colon to inflate. If the airflow is too strong, air will be pumped into the stomach of the mouse. No additional lubrication is required.</li>
	<li>Carefully insert the rigid endoscope sheath into the rectum. Generally, the endoscope can be inserted up to 3 cm, at which point the colon in mice curves and is not accessible to the rigid endoscope.</li>
	<li>A common difficulty during endoscopy procedures is blockage of access to the lumen of the colon due to fecal matter. Avoid this by gently massaging of the belly of mice prior to the procedure to encourage defecation, or carefully maneuvering the endoscope around the fecal matter during the procedure. Peristalsis can also occur, during which the endoscope should be held in position until the colon musculature relaxes.</li>
	<li>Initiate video recording at any stage of the endoscopy procedure. Disease scoring can be recorded by an experienced assistant during the procedure, or at a later time point from the video files.</li>
	<li>Following the endoscopic exam, return the mice to their cage and monitor them during recovery from anesthesia. Animals are generally awake and mobile within 2 min following removal from the isoflurane administering nose cone.</li>
	<li>Ensure that these procedures are performed by an experienced scientist. Each endoscopy procedure will take approximately 2 min per mouse.</li>
</ol>
6. Disease Scoring
<ol>
	<li>To monitor colitis, score videos for the Murine Endoscopic Index of Colitis Severity (MEICS)16, which documents changes in (i) the thickness of the colon wall indicated by transparency, (ii) stool consistency, (iii) blood vessel integrity and presence, (iv) ulcers and areas of regeneration that present in a granular fashion, (v) bleeding indicated by fibrin deposits (Figure 5a).</li>
	<li>To monitor tumor burden, score videos for tumor incidence and size. Tumor size is determined by the diameter of the colonic lumen occupied by the tumor16 (Figure 5b). It is common to use both colitis and tumor scoring parameters for a single mouse. Using endoscopy, individual tumors and the health of the colonic mucosa can be monitored over time, providing a read-out for the success of new therapeutics in a single animal.</li>
	<li>(Optional) Still images can be extracted from the videos for generation of representative figures (Figure 6).</li>
</ol>

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The authors have nothing to disclose.

The three protocols that are described outline methods of reliable and reproducible induction of colonic disease pathology in mice. When combined with routine endoscopic monitoring and the intervention strategies outlined here, these protocols will provide powerful pre-clinical insight into the efficacy of therapeutics. Our laboratories routinely use all of these protocols to monitor the success of novel therapeutics10,23,24.
There are a number of considerations when choosing a pre-clinical animal model to test new therapeutics. These include relevance of the model to the human disease, and the contribution of the tumor microenvironment to the proposed action of the therapeutic target. Here we provide three protocols for therapeutic intervention in established intestinal disease models. These models are reproducible and the delivery of reagents to induce disease is easy to manage. Importantly, the models are highly relevant to multiple facets and stages of colitis onset, and of tumor initiation and progression. Researchers should take into consideration the genetic background of the mouse strains used when designing experiments, as the susceptibility to disease induced by DSS and/or AOM can vary considerably25. In addition, different microbial communities may have different metabolic capacities in the context of AOM, which is metabolized by bacteria. We caution against using different cohorts of mice that were born into different animal facilities (including commercial vendors) in a single experiment. Similarly, the different microflora in mice used from different facilities may elicit different host responses to DSS-induced epithelial barrier damage11. Moreover, the appropriate analysis of tissue (for example RNA purification) should also be considered, since the ability of DSS to inhibit reverse transcriptase will impact on subsequent molecular analysis26,27.
Mouse endoscopy is a cutting edge technique to repeatedly monitor disease onset and progression in an individual mouse. The ability to record videos and extract still images permits easy monitoring of multiple disease parameters and tumors. In addition to improving animal welfare, endoscopic monitoring also reduces the need for multiple cohorts of experimental mice, which traditionally were culled at different time-points to track disease outcome. The MEICS scoring system is not a substitute for histopathological analysis, but provides an alternative means to monitor animal health and mucosal damage in live mice. Mouse endoscopy is a specialized laboratory technique, and all procedures should be performed by trained personnel to ensure appropriate manipulation and handling of the mice, as well as to provide consistent quality in the images used for disease scoring. In the hands of qualified personal, we have found that endoscopy induces little or no damage to the tumors that would cause intra-tumoral bleeding. For the therapeutic protocols outlined, we consider endoscopy highly advantageous, since it provides a way to determine the initial tumor burden, and allows us to group cohorts of animals with similar tumor burdens prior to the administration of a therapeutic drug. Sequential monitoring of the mice enables researchers to determine the efficacy of novel therapies early on, with the option of terminating unsuccessful experiments in a timely manner.
As our understanding of inflammatory bowel disease and colorectal cancers advance, new targets for therapy will be identified. Appropriate animal models will be integral to ensuring that the most promising new therapies are moved towards clinical trials.

Colorectal cancer (CRC) is the 4th most common cause of malignancy worldwide1. Despite the significant progress in our understanding of the familial basis of this disease, genetic predisposition only contributes to ~20% of CRC cases2. The remainder are attributed to numerous extrinsic and environmental factors, including chronic inflammation. In humans, the link between chronic inflammation and colon cancer is evident in ulcerative colitis (UC) patients, who have a greater risk of developing colitis-associated colon cancer (CAC), depending on the duration, extent and severity of the inflammatory disease3-5. Accordingly, novel therapies are in development to control the immune response and the associated production of growth promoting factors by the inflammatory tumor microenvironment6-8. There is an increasing requirement for appropriate pre-clinical animal models to characterize the therapeutic efficacy of these drugs against the development and progression of disease.
Mouse models have unequivocally demonstrated that the inflammatory microenvironment contributes to CRC progression, even in the absence of overt inflammation9,10. These models include the use of the polysaccharide dextran sulfate sodium (DSS), provided in the drinking water of mice, to model epithelial injury and acute and chronic inflammatory bowel disease (IBD)11,12. Although the mechanism by which DSS induces mucosal damage and colitis is not completely understood, some studies suggest that DSS inhibits cellular reverse transcriptase and ribonuclease activities within cells, or promotes the formation of nano-lipid complexes that fuse with the colonic membrane leading to epithelial damage13,14. Modifications to the standard DSS model have also provided significant insight into the mechanisms by which colonic epithelial cells maintain tissue homeostasis and regulate mucosal immune responses15.
Intraperitoneal administration of Azoxymethane (AOM) alone, or in combination with DSS, provides a model for examining the interplay between somatic mutations in the epithelial mucosa and the inflammatory and stromal microenvironment16,17. AOM is a metabolite of the carcinogen 1,2-dimethylhydrazine (DMH) that does not directly result in DNA mutations. Instead, AOM is hydrolyzed to methylazoxymethanol (MAM) by the cytochrome isoform CYP2E1 in the liver, where MAM is conjugated with glucuronic acid and then transported to the intestine through bile secretions18. It is thought that the bacterial &#946;-glucuronidase contributes to the degradation of MAM resulting in DNA alkylation and the accumulation of mutations in epithelial cells19. Most AOM-induced colonic tumors harbor missense mutations in the gene encoding &#946;-catenin, rendering the protein resistant to proteasomal degradation, which results in aberrant activation of the canonical Wnt-signaling pathway20. When the activity of AOM is combined with the mucosal damage elicited by DSS, the ensuing wound healing response creates a microenvironment that is conducive to the growth and expansion of the mutagenized epithelium. In a variation of this model, repetitive administration of AOM alone over a period of several weeks can be used to model sporadic colorectal cancer, in the absence of DSS-induced colitis10,17. These two complimentary models provide experimental settings to study CAC and sporadic CRC respectively, both of which are associated with a pro-inflammatory tumor microenvironment10.
The use of serial endoscopy in mice was pioneered by Becker and colleagues21, and enables longitudinal monitoring of colitis and tumor progression. Here we provide three pre-clinical protocols based on DSS-induced mucosal damage and/or AOM-mediated tumor induction to reproducibly induce specific colonic pathologies. The first protocol describes inducing acute mucosal damage in response to DSS administration to elicit many of the histopathological features associated with IBD. The second protocol is based on three consecutive cycles of DSS administration to mimic the flares of inflammation commonly observed in IBD patients, and can be carried out in conjunction with AOM-induced mutations. The final protocol is based on AOM-induced sporadic epithelial mutations. For each of these protocols, we expand on the relevant standard procedures to include prophylactic and therapeutic intervention methods that we have developed to monitor the efficacy of new drugs.

<table border="0" cellpadding="0" cellspacing="0" width="1021">
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Name of Material/ Equipment</td>
			<td style="width:112px;">Company</td>
			<td style="width:119px;">Catalog Number</td>
			<td style="width:509px;">Comments/Description</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:281px;">Dextran Sulfate Sodium (MW 36,000-50,000)</td>
			<td style="width:112px;">MP Biochemicals</td>
			<td style="width:119px;">160110</td>
			<td>Requires batch testing.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Azoxymethane</td>
			<td style="width:112px;">Sigma</td>
			<td style="width:119px;">A5486-100MG</td>
			<td>Requires batch testing.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Vanilla Protein Shake</td>
			<td style="width:112px;">N/A</td>
			<td style="width:119px;">N/A</td>
			<td>Available from hospital pharmacies.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Isoflourane</td>
			<td style="width:112px;">PPC</td>
			<td style="width:119px;">M60303</td>
			<td>This is a restricted reagent, which should be stored under lock and key.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">70% Ethanol</td>
			<td style="width:112px;">N/A</td>
			<td style="width:119px;">N/A</td>
			<td>Standard lab reagent.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;"></td>
			<td style="width:112px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Coloview miniendoscopic system</td>
			<td style="width:112px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Endovision Tricam</td>
			<td style="width:112px;">Karl Storz</td>
			<td style="width:119px;">20212001-020</td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:281px;">Xenon 175 light source with anti-fog pump</td>
			<td style="width:112px;">Karl Storz</td>
			<td style="width:119px;">20134001</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">HOPKINS straight Forward Telescope</td>
			<td style="width:112px;">Karl Storz</td>
			<td style="width:119px;">64301AA</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Endoscopic Sheath (total diameter 3 mm)</td>
			<td style="width:112px;">Kalr Stroz</td>
			<td style="width:119px;">61029C</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Fubre Optic Light Cable</td>
			<td style="width:112px;">Kalr Stroz</td>
			<td style="width:119px;">69495ND</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Computer and media player software</td>
			<td style="width:112px;">MAC, imovies</td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:281px;">Scale</td>
			<td style="width:112px;">Any</td>
			<td style="width:119px;"></td>
			<td>Any scale suitable for weighing mice.</td>
		</tr>
	</tbody>
</table>

non-invasive assessment of the efficacy of new therapeutics for intestinal pathologies using serial endoscopic imaging of live mice

Animal models of inflammatory bowel disease (IBD) and colorectal cancer (CRC) have provided significant insight into the cell intrinsic and extrinsic mechanisms that contribute to the onset and progression of intestinal diseases. The identification of new molecules that promote these pathologies has led to a flurry of activity focused on the development of potential new therapies to inhibit their function. As a result, various pre-clinical mouse models with an intact immune system and stromal microenvironment are now heavily used. Here we describe three experimental protocols to test the efficacy of new therapeutics in pre-clinical models of (1) acute mucosal damage, (2) chronic colitis and/or colitis-associated colon cancer, and (3) sporadic colorectal cancer. We also outline procedures for serial endoscopic examination that can be used to document the therapeutic response of an individual tumor and to monitor the health of individual mice. These protocols provide complementary experimental platforms to test the effectiveness of therapeutic compounds shown to be well tolerated by mice.

Weight-loss is used as a standard parameter to monitor for disease associated with colitis, which is routinely used to monitor the overall health of mice. Animals generally maintain their weight while DSS-containing water is administered, and only start to loose weight when they are returned to normal drinking water. Acceptable weight-loss parameters should be established in accordance with the institution&#8217;s animal ethics committee. In order to prevent the dehydration associated with prolonged diarrhea, use the routine provision of mash (food pellets mashed and mixed with drinking water) supplemented with a protein shake in addition to normal drinking water.
As an alternative anesthesia, ketamine/xylazine or similar agents can be used, if isoflurane equipment is not available. Due to the rigid nature of the endoscope, these procedures only allow for visualization of the most distal 3 cm of the mouse colon. Newer endoscopes with additional capabilities (including flexibility and fluorescence) are available depending on the needs of the experiment. However, since the deleterious effects of DSS are primarily limited to the distal colon of mice, with milder pathology observed in the middle colon, the rigid endoscope does not hinder monitoring of the mucosal health of individual mice. Although we describe a protocol for prophylactic treatment of acute DSS-induced colitis, this protocol can easily be modified to test intervention treatment strategies. The efficacy of a drug designed to alleviate epithelial damage and colitis can be monitored longitudinally in individual mice and quantified based on the scoring parameters described (Figure 5). This is advantageous over traditional experimental designs, which require culling of mice at specific time points during the experimental protocol, and does not permit characterization of the disease response to a treatment over time.
Clinical studies in humans have highlighted considerable variability in how different tumors in an individual patient respond to treatments. The procedures that are described here provide a means to monitor overall tumor burden, as well as the treatment response of individual tumors over the course of an experiment. It is important to consider that the intervention protocols that are outlined for the cancer models do not take into account the effects of a therapy on tumor initiation. Prophylactic protocols, with the treatment provided prior to when tumors become visible by endoscopy, are required to obtain this information. The protocols outlined here provide information on therapeutic effects on the on the progression (measured by tumor size) of individual tumors. Tumor regression may also be indicated by a reduction in the number of visible tumors.
<img alt="Figure 1" src="/files/ftp_upload/52383/52383fig1highres.jpg" /> 
Figure 1: Monitoring the efficacy of a prophylactic treatment therapy in a model of acute colonic damage. The experimental protocol (a) requires 8 days from start to completion. Therapeutics are administered (b) from Day 1 for prophylactic treatments. DSS is provided in the drinking water (c) from Day 3 of the experimental protocol. Endoscopy is performed (d) to monitor the disease progression in the animals. Suggested timepoints include Day 0 (untreated) and Day 2 (health monitoring), Day 5 and 8 (to determine disease burden). The experiment is terminated (e) the morning of Day 8. In a wild-type mouse (f) the progression of disease increases over time.
<img alt="Figure 2" src="/files/ftp_upload/52383/52383fig2highres.jpg" /> 
Figure 2: Monitoring the efficacy of intervention therapy in a model of colitis-associated cancer. The experimental protocol (a) requires 72 days from start to completion. Therapeutics (b) are administered to mice with established tumors from Day 46 for intervention treatments. AOM (c) is injected on Day 1, and DSS is provided in the drinking water over the course of three cycles of the experimental protocol, beginning on Day 8. Endoscopy (d) is performed to monitor the disease progression in the animals. Suggested timepoints include Day 0 (untreated), Day 20 (health monitoring), and Day 40 (to group animals according to tumor burden). Endoscopy is performed weekly over the course of the therapeutic treatment to monitor disease outcomes. The experiment (e) is terminated the morning of Day 72. In a wild-type mouse (f) tumor burden increases from Day 40 onwards.
<img alt="Figure 3" src="/files/ftp_upload/52383/52383fig3highres.jpg" /> 
Figure 3: Monitoring the efficacy of intervention therapy in a model of spontaneous colorectal cancer. The experimental protocol (a) requires &#62;50 weeks from start to completion. Therapeutics (b) are administered to mice with established tumors for intervention treatments. AOM (c) is injected on Day 1, and weekly thereafter for 6 consecutive injections over the course of the experimental protocol. Endoscopy (d) is performed to monitor the disease progression in the animals. Suggested timepoints include Day 0 (untreated) and Week 8 (tumor monitoring) and biweekly there after (to establish tumor burden). Endoscopy is performed weekly over the course of treatment to monitor therapeutic outcomes. The experiment (e) is terminated in Week 50. In a wild-type mouse (f) tumor burden increases from Week 40 onwards.
<img alt="Figure 4" src="/files/ftp_upload/52383/52383fig4highres.jpg" width="650" /> 
Figure 4: Equipment set-up. The experimental set-up (a) for the endoscopic unit, with individual pieces of equipment indicated. The rigid endoscope (b), with individual components indicated. Scale bar = 2.5 cm. <a href="https://www.jove.com/files/ftp_upload/52383/52383fig4highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" src="/files/ftp_upload/52383/52383fig5highres.jpg" width="650" /> 
Figure 5: Scoring disease parameters by endoscopy. An outline (a) of the Murine Endoscopic Index of Colitis Severity (MEICS). An outline (b) of the individual tumor scoring parameters. <a href="https://www.jove.com/files/ftp_upload/52383/52383fig5highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" src="/files/ftp_upload/52383/52383fig6highres.jpg" width="650" /> 
Figure 6: Representative therapeutic treatments. Representative weight-loss, endoscopic images and scores for: (a) Acute DSS-induced mucosal damage. (b) Tumors that developed following the AOM/DSS protocol. (c) Tumors that developed following the sequential AOM protocol. N = 3 mice per group. *P &#60;0.05, ***P &#60;0.001 (Student&#8217;s T-test). <a href="https://www.jove.com/files/ftp_upload/52383/52383fig6highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Non-invasive Assessment of the Efficacy of New Therapeutics for Intestinal Pathologies Using Serial Endoscopic Imaging of Live Mice at JoVE.com

Non-invasive Assessment of the Efficacy of New Therapeutics for Intestinal Pathologies Using Serial Endoscopic Imaging of Live Mice

We describe methods for longitudinal monitoring of the efficacy of therapeutics for the treatment of colonic pathologies in mice using a rigid endoscope. This protocol can be readily used for the characterization of the therapeutic response of an individual tumor in live mice and also for monitoring potential disease relapse.

Animal models of inflammatory bowel disease (IBD) and colorectal cancer (CRC) have provided significant insight into the cell intrinsic and extrinsic ...

non-invasive-assessment-efficacy-new-therapeutics-for-intestinal

Research

JoVE Journal

Medicine

Magnetic Resonance Derived Myocardial Strain Assessment Using Feature Tracking

Purpose: An accurate and practical method to measure parameters like strain in myocardial tissue is of great clinical value, since it has been shown, that strain is a more sensitive and earlier marker for contractile dysfunction than the frequently used parameter EF. Current technologies for CMR are time consuming and difficult to implement in clinical practice. Feature tracking is a technology that can lead to more automization and robustness of quantitative analysis of medical images with less time consumption than comparable methods.
Methods: An automatic or manual input in a single phase serves as an initialization from which the system starts to track the displacement of individual patterns representing anatomical structures over time. The specialty of this method is that the images do not need to be manipulated in any way beforehand like e.g. tagging of CMR images.
Results: The method is very well suited for tracking muscular tissue and with this allowing quantitative elaboration of myocardium and also blood flow.
Conclusions: This new method offers a robust and time saving procedure to quantify myocardial tissue and blood with displacement, velocity and deformation parameters on regular sequences of CMR imaging. It therefore can be implemented in clinical practice.

An accurate and practical method to measure parameters like strain in myocardial tissue is of great clinical value, since it has been shown, that strain is a more sensitive and earlier marker for contractile dysfunction than the frequently used parameter EF.

Purpose: An accurate and practical method to measure parameters like strain in myocardial tissue is of great clinical value, since it has been shown, that ...

Non-invasive Imaging of Acute Allograft Rejection after Rat Renal Transplantation Using 18F-FDG PET

The number of patients with end-stage renal disease, and the number of kidney allograft recipients continuously increases. Episodes of acute cellular allograft rejection (AR) are a negative prognostic factor for long-term allograft survival, and its timely diagnosis is crucial for allograft function 1. At present, AR can only be definitely diagnosed by core-needle biopsy, which, as an invasive method, bares significant risk of graft injury or even loss. Moreover, biopsies are not feasible in patients taking anticoagulant drugs and the limited sampling site of this technique may result in false negative results if the AR is focal or patchy. As a consequence, this gave rise to an ongoing search for new AR detection methods, which often has to be done in animals including the use of various transplantation models.
Since the early 60s rat renal transplantation is a well-established experimental method for the examination and analysis of AR 2. We herein present in addition small animal positron emission tomography (PET) using 18F-fluorodeoxyglucose (FDG) to assess AR in an allogeneic uninephrectomized rat renal transplantation model and propose graft FDG-PET imaging as a new option for a non-invasive, specific and early diagnosis of AR also for the human situation 3. Further, this method can be applied for follow-up to improve monitoring of transplant rejection 4.

Non-invasive Imaging of Acute Allograft Rejection after Rat Renal Transplantation Using 18F-FDG PET

We herein present a rat renal transplantation model to non-invasively assess acute allograft rejection using positron emission tomography with 18F-fluorodeoxyglucose.

The number of patients with end-stage renal  disease, and the number of kidney allograft recipients continuously increases.  Episodes of acute cellular ...

Non-invasive Optical Measurement of Cerebral Metabolism and Hemodynamics in Infants

Perinatal brain injury remains a significant cause of infant mortality and morbidity, but there is not yet an effective bedside tool that can accurately screen for brain injury, monitor injury evolution, or assess response to therapy. The energy used by neurons is derived largely from tissue oxidative metabolism, and neural hyperactivity and cell death are reflected by corresponding changes in cerebral oxygen metabolism (CMRO2). Thus, measures of CMRO2 are reflective of neuronal viability and provide critical diagnostic information, making CMRO2 an ideal target for bedside measurement of brain health.
Brain-imaging techniques such as positron emission tomography (PET) and single-photon emission computed tomography (SPECT) yield measures of cerebral glucose and oxygen metabolism, but these techniques require the administration of radionucleotides, so they are used in only the most acute cases.
Continuous-wave near-infrared spectroscopy (CWNIRS) provides non-invasive and non-ionizing radiation measures of hemoglobin oxygen saturation (SO2) as a surrogate for cerebral oxygen consumption. However, SO2 is less than ideal as a surrogate for cerebral oxygen metabolism as it is influenced by both oxygen delivery and consumption. Furthermore, measurements of SO2 are not sensitive enough to detect brain injury hours after the insult 1,2, because oxygen consumption and delivery reach equilibrium after acute transients 3. We investigated the possibility of using more sophisticated NIRS optical methods to quantify cerebral oxygen metabolism at the bedside in healthy and brain-injured newborns. More specifically, we combined the frequency-domain NIRS (FDNIRS) measure of SO2 with the diffuse correlation spectroscopy (DCS) measure of blood flow index (CBFi) to yield an index of CMRO2 (CMRO2i) 4,5.
With the combined FDNIRS/DCS system we are able to quantify cerebral metabolism and hemodynamics. This represents an improvement over CWNIRS for detecting brain health, brain development, and response to therapy in neonates. Moreover, this method adheres to all neonatal intensive care unit (NICU) policies on infection control and institutional policies on laser safety. Future work will seek to integrate the two instruments to reduce acquisition time at the bedside and to implement real-time feedback on data quality to reduce the rate of data rejection.

We combined frequency-domain near-infrared spectroscopy measures of cerebral hemoglobin oxygenation with diffuse correlation spectroscopy measures of cerebral blood flow index to estimate an index of oxygen metabolism. We tested the utility of this measure as a bedside screening tool to evaluate the health and development of the newborn brain.

Perinatal brain injury remains a significant cause of infant mortality  and morbidity, but there is not yet an effective bedside tool that can  accurately ...

Intranasal Administration of CNS Therapeutics to Awake Mice

Intranasal administration is a method of delivering therapeutic agents to the central nervous system (CNS). It is non-invasive and allows large molecules that do not cross the blood-brain barrier access to the CNS. Drugs are directly targeted to the CNS with intranasal delivery, reducing systemic exposure and thus unwanted systemic side effects1. Delivery from the nose to the CNS occurs within minutes along both the olfactory and trigeminal neural pathways via an extracellular route and does not require drug to bind to any receptor or axonal transport2. Intranasal delivery is a widely publicized method and is currently being used in human clinical trials3.
Intranasal delivery of drugs in animal models allows for initial evaluation of pharmacokinetic distribution and efficacy. With mice, it is possible to administer drugs to awake (non-anesthetized) animals on a regular basis using a specialized intranasal grip. Awake delivery is beneficial because it allows for long-term chronic dosing without anesthesia, it takes less time than with anesthesia, and can be learned and done by many people so that teams of technicians can dose large numbers of mice in short periods. Efficacy of therapeutics administered intranasally in this way to mice has been demonstrated in a number of studies including insulin in diabetic mouse models 4-6 and deferoxamine in Alzheimer's mouse models. 7,8
The intranasal grip for mice can be learned, but is not easy and requires practice, skill, and a precise grip to effectively deliver drug to the brain and avoid drainage to the lung and stomach. Mice are restrained by hand using a modified scruff in the non-dominant hand with the neck held parallel to the floor, while drug is delivered with a pipettor using the dominant hand. It usually takes 3-4 weeks of acclimating to handling before mice can be held with this grip without a stress response. We have prepared this JoVE video to make this intranasal delivery technique more accessible.

A method to intranasally administer drugs to awake mice for the purpose of targeting the brain is described. This method allows for repeat dosing over long periods using intranasal administration of drug without anesthesia, and nose-to-brain delivery with minimal systemic exposure.

Intranasal administration is a method of delivering  therapeutic agents to the central nervous system (CNS). It is  non-invasive and allows large ...

Non-invasive Assessment of Microvascular and Endothelial Function

The authors have utilized capillaroscopy and forearm blood flow techniques to investigate the role of microvascular dysfunction in pathogenesis of cardiovascular disease. Capillaroscopy is a non-invasive, relatively inexpensive methodology for directly visualizing the microcirculation. Percent capillary recruitment is assessed by dividing the increase in capillary density induced by postocclusive reactive hyperemia (postocclusive reactive hyperemia capillary density minus baseline capillary density), by the maximal capillary density (observed during passive venous occlusion). Percent perfused capillaries represents the proportion of all capillaries present that are perfused (functionally active), and is calculated by dividing postocclusive reactive hyperemia capillary density by the maximal capillary density. Both percent capillary recruitment and percent perfused capillaries reflect the number of functional capillaries. The forearm blood flow (FBF) technique provides accepted non-invasive measures of endothelial function: The ratio FBFmax/FBFbase is computed as an estimate of vasodilation, by dividing the mean of the four FBFmax values by the mean of the four FBFbase values. Forearm vascular resistance at maximal vasodilation (FVRmax) is calculated as the mean arterial pressure (MAP) divided by FBFmax. Both the capillaroscopy and forearm techniques are readily acceptable to patients and can be learned quickly.
The microvascular and endothelial function measures obtained using the methodologies described in this paper may have future utility in clinical patient cardiovascular risk-reduction strategies. As we have published reports demonstrating that microvascular and endothelial dysfunction are found in initial stages of hypertension including prehypertension, microvascular and endothelial function measures may eventually aid in early identification, risk-stratification and prevention of end-stage vascular pathology, with its potentially fatal consequences.

Capillaroscopy is a non-invasive, relatively inexpensive methodology for directly visualizing the microcirculation. The forearm blood flow technique provides accepted non-invasive measures of endothelial function.

The authors have utilized capillaroscopy and forearm blood flow techniques to investigate the role of microvascular dysfunction in pathogenesis of ...

Non-invasive Imaging and Analysis of Cerebral Ischemia in Living Rats Using Positron Emission Tomography with 18F-FDG

Stroke is the third leading cause of death among Americans 65 years of age or older1. The quality of life for patients who suffer from a stroke fails to return to normal in a large majority of patients2, which is mainly due to current lack of clinical treatment for acute stroke. This necessitates understanding the physiological effects of cerebral ischemia on brain tissue over time and is a major area of active research. Towards this end, experimental progress has been made using rats as a preclinical model for stroke, particularly, using non-invasive methods such as 18F-fluorodeoxyglucose (FDG) coupled with Positron Emission Tomography (PET) imaging3,10,17. Here we present a strategy for inducing cerebral ischemia in rats by middle cerebral artery occlusion (MCAO) that mimics focal cerebral ischemia in humans, and imaging its effects over 24 hr using FDG-PET coupled with X-ray computed tomography (CT) with an Albira PET-CT instrument. A VOI template atlas was subsequently fused to the cerebral rat data to enable a unbiased analysis of the brain and its sub-regions4. In addition, a method for 3D visualization of the FDG-PET-CT time course is presented. In summary, we present a detailed protocol for initiating, quantifying, and visualizing an induced ischemic stroke event in a living Sprague-Dawley rat in three dimensions using FDG-PET.

Non-invasive Imaging and Analysis of Cerebral Ischemia in Living Rats Using Positron Emission Tomography with 18F-FDG

Brain damage resulting from cerebral ischemia may be non-invasively imaged and studied in rats using pre-clinical positron emission tomography coupled with the injectable radioactive probe, 18F-fluorodeoxyglucose. Further, the use of modern software tools that include volume of interest (VOI) brain templates dramatically increase the quantitative information gleaned from these studies.

Stroke is the third leading cause of death among Americans 65 years of age or older1. The quality of life for patients who suffer from a stroke fails to ...

Murine Model for Non-invasive Imaging to Detect and Monitor Ovarian Cancer Recurrence

Epithelial ovarian cancer is the most lethal gynecologic malignancy in the United States. Although patients initially respond to the current standard of care consisting of surgical debulking and combination chemotherapy consisting of platinum and taxane compounds, almost 90% of patients recur within a few years. In these patients the development of chemoresistant disease limits the efficacy of currently available chemotherapy agents and therefore contributes to the high mortality. To discover novel therapy options that can target recurrent disease, appropriate animal models that closely mimic the clinical profile of patients with recurrent ovarian cancer are required. The challenge in monitoring intra-peritoneal (i.p.) disease limits the use of i.p. models and thus most xenografts are established subcutaneously. We have developed a sensitive optical imaging platform that allows the detection and anatomical location of i.p. tumor mass. The platform includes the use of optical reporters that extend from the visible light range to near infrared, which in combination with 2-dimensional X-ray co-registration can provide anatomical location of molecular signals. Detection is significantly improved by the use of a rotation system that drives the animal to multiple angular positions for 360 degree imaging, allowing the identification of tumors that are not visible in single orientation. This platform provides a unique model to non-invasively monitor tumor growth and evaluate the efficacy of new therapies for the prevention or treatment of recurrent ovarian cancer.

We describe a non-invasive animal imaging platform that allows the detection, quantification, and monitoring of ovarian cancer growth and recurrence. This intra-peritoneal xenograft model mimics the clinical profile of patients with ovarian cancer.

Epithelial ovarian cancer is the most lethal gynecologic malignancy in the United States. Although patients initially respond to the current standard of ...

Murine Endoscopy for In Vivo Multimodal Imaging of Carcinogenesis and Assessment of Intestinal Wound Healing and Inflammation

Mouse models are widely used to study pathogenesis of human diseases and to evaluate diagnostic procedures as well as therapeutic interventions preclinically. However, valid assessment of pathological alterations often requires histological analysis, and when performed ex vivo, necessitates death of the animal. Therefore in conventional experimental settings, intra-individual follow-up examinations are rarely possible. Thus, development of murine endoscopy in live mice enables investigators for the first time to both directly visualize the gastrointestinal mucosa and also repeat the procedure to monitor for alterations. Numerous applications for in vivo murine endoscopy exist, including studying intestinal inflammation or wound healing, obtaining mucosal biopsies repeatedly, and to locally administer diagnostic or therapeutic agents using miniature injection catheters. Most recently, molecular imaging has extended diagnostic imaging modalities allowing specific detection of distinct target molecules using specific photoprobes. In conclusion, murine endoscopy has emerged as a novel cutting-edge technology for diagnostic experimental in vivo imaging and may significantly impact on preclinical research in various fields.

Murine Endoscopy for In Vivo Multimodal Imaging of Carcinogenesis and Assessment of Intestinal Wound Healing and Inflammation

Small animal imaging techniques allow serial diagnostic examinations and therapeutic interventions in vivo. Recently, the scope of applications has significantly widened and currently includes assessment of colonic tumor development, wound healing and monitoring of inflammation. This protocol illustrates these diverse potential applications of murine endoscopy.

Mouse models are widely used to study pathogenesis of human diseases and to evaluate diagnostic procedures as well as therapeutic interventions ...

Non-invasive Assessment of Dorsiflexor Muscle Function in Mice

Assessment of skeletal muscle contractile function is an important measurement for both clinical and research purposes. Numerous conditions can negatively affect skeletal muscle. This can result in a loss of muscle mass (atrophy) and/or loss of muscle quality (reduced force per unit of muscle mass), both of which are prevalent in chronic disease, muscle-specific disease, immobilization, and aging (sarcopenia). Skeletal muscle function in animals can be evaluated by a range of different tests. All tests have limitations related to the physiological testing environment, and the selection of a specific test often depends on the nature of the experiments. Here, we describe an in vivo, non-invasive technique involving a helpful and easy assessment of force frequency-curve (FFC) in mice that can be performed on the same animal over time. This permits monitoring of disease progression and/or efficacy&#160;of a potential therapeutic treatment.

Measurement of rodent skeletal muscle contractile function is a useful tool that can be used to track disease progression as well as efficacy of therapeutic intervention. We describe here the non-invasive, in vivo assessment of the dorsiflexor muscles that can be repeated over time in the same mouse.

Assessment of skeletal muscle contractile function is an important measurement for both clinical and research purposes. Numerous conditions can negatively ...

Assessment and Characterization of Hyaloid Vessels in Mice

In the eye, the embryonic hyaloid vessels nourish the developing lens and retina and regress when the retinal vessels develop. Persistent or failed regression of hyaloid vessels can be seen in diseases such as persistent hyperplastic primary vitreous (PHPV), leading to an obstructed light path and impaired visual function. Understanding the mechanisms underlying the hyaloid vessel regression may lead to new molecular insights into the vascular regression process and potential new ways to manage diseases with persistent hyaloid vessels. Here we describe the procedures for imaging hyaloid in live mice with optical coherence tomography (OCT) and fundus fluorescein angiography (FFA) and a detailed technical protocol of isolating and flat-mounting hyaloid ex vivo for quantitative analysis. Low-density lipoprotein receptor-related protein 5 (LRP5) knockout mice were used as an experimental model of persistent hyaloid vessels, to illustrate the techniques. Together, these techniques may facilitate a thorough assessment of hyaloid vessels as an experimental model of vascular regression and studies on the mechanism of persistent hyaloid vessels.

This protocol describes both in vivo and ex vivo methods to fully visualize and characterize hyaloid vessels, a model of vascular regression in mouse eyes, using optical coherence tomography and fundus fluorescein angiography for the live imaging and ex vivo isolation and subsequent flat mount of hyaloid for quantitative analysis.

In the eye, the embryonic hyaloid vessels nourish the developing lens and retina and regress when the retinal vessels develop. Persistent or failed ...