We thank Dr. Harvey Hensley for his expert technical support.  This work benefited from the use of the following Fox Chase Cancer Center (FCCC) facilities: Laboratory of Animal Facility and Small Animal Imaging Facility.  This work was supported in part by the Ovarian Cancer SPORE at FCCC/UPenn (P50 CA083638), the FCCC core grant (P30 CA006927), and the Ovarian Cancer Research Fund.

I. Preparation of Ovarian Tumor Cells
<ol>
<li>	Grow ovarian cancer cell lines expressing luciferase in culture. Sources of luciferase can be Firefly, Renilla, or other species. Cells expressing fluorescent proteins can also be used. For this demonstration we use an ovarian cancer cell line, OVCAR5, expressing firefly luciferase.</li>
<li>	Harvest cells using routine cell culture technique.</li>
<li>	Keep the cell suspension (10,000 cells/&mu;L) in phosphate buffered saline (PBS) on ice until time of injection.</li>
</ol>

II. Intrabursal Injection
This procedure requires assistance from a second person. All surgical procedures are conducted under aseptic conditions. This includes wearing surgical attire and using sterile surgical instruments, syringe, and needles.
<ol>
<li>	Prepare the anesthetic solution by mixing 3 mL of ketamine hydrochloride (100 mg/mL), 1.6 mL of xylazine hydrochloride (100 mg/mL), 1.5 mL of acepromazine (10 mg/mL), and 20 mL of 0.9% sodium chloride.</li>
<li>	Check the animal's identification number and observable health. Anesthetize the animal with prepared ketamine-xylazine-acepromazine anesthesia via intraperitoneal (i.p.) injection with a dose volume of 8~9 mL/kg body weight (BW).</li>
<li>	Confirm that the animal is under an acceptable plain of anesthesia by performing a toe pinch with forceps or fingers to the animal's hind paws. If there is pedal reflex, wait for a deeper plain of anesthesia until the animal is unresponsive to this procedure.</li>
<li>	Lay the animal dorsal side up on a sterile gauze pad with its head facing away and its tail facing towards you. The point of incision is located to the left or right of the midline and above the ovaries. Shave or wet the fur with 70% alcohol at the incision point.</li>
<li>	Lift the wetted skin using forceps and make a small incision with the scissor at the dorsomedial position and directly above the ovarian fat pad. The ovarian fat pad should be visible beneath the surface of the peritoneal wall. Fat pad is easily recognizable by its white color in contrast to the dark pink tissue surrounding it.</li>
<li>	Gently lift the peritoneal wall lining and make a small incision as described above (5).</li>
<li>	Place a sterile soaked saline gauze pad on the midline adjacent to the incision. Locate the ovarian fat pad and gently pull it out and rest it onto the gauze. Stabilize the ovary by clamping the fat pad with a bulldog clip. Under a dissecting microscope, position the ovary as to allow for the insertion of the needle (30 gauge, G) into the oviduct tubule bend leading to the bursa. When the needle is inserted into the proper position, it should be visible under the bursa.</li>
<li>	Gently push the plunger of the syringe to inject 5 &mu;L of cell suspension between the bursa and the ovary while the syringe is positioned to injection site. This step requires two people. One person pushes the plunger while the other person maintains positioning of needle. Remove the needle quickly to seal the puncture site but gently enough not to tear the bursa and tubule. The bursa should appear to be slightly distended with proper injection.</li>
<li>	Release the fat pad from the bulldog clip and gently replace the reproductive tract and fat pad back into the peritoneal cavity. Gently close the body wall by pulling the upper peritoneal lining over the lower lining. Close the skin with surgical staples or wound clips.</li>
<li>	Place the recovering animal back in its cage and provide a safe heat source to avoid hypothermia and speed up recovery. Monitor the breathing rate and ease, the return of muscle tone, and the ability to voluntarily move. These are all good indicators of the progression towards recovery. Staples or wound clips can be removed 7 or more days post surgery.</li>
</ol>

III. Oral Gavage Administration
<ol>
<li>	Use an 18~20 G gavage needle or feeding tube with a rounded tip. The gavage needle should be no longer than the distance from the tip of the animal's head to its last rib.</li>
<li>	Check the animals' identification number and observable health. Gently scruff the animal by grasping the skin over the shoulders with thumb and fingers. The restraint should be just firm enough for the fore limbs to be extended to each side and out of the way. The animal should not be able to grasp at the needle.</li>
<li>	Gently pull back the animal's head with your index finger, forming a straight line through the neck and esophagus. Support the animal's back with the inside of your thumb.</li>
<li>	Gently and without force, insert the gavage needle at either side of the mouth and over the tongue. In one smooth motion, the needle should pass against the roof of the mouth and down the esophagus. Gravity should guide the needle down without meeting resistance. If there is any resistance, remove the needle and start again. The animal's gag and swallow reflex may be triggered during insertion. However, there should be no resistance or gasping from the animal. It is important to make sure that the animal is breathing when the needle is in place by checking the movement of the nostrils and chest.</li>
<li>	Slowly push plunger of the syringe to dispense the dose volume.</li>
<li>	Gently remove the gavage needle at the same angle and pathway as the way it was inserted down the esophagus.</li>
<li>	Return the animal to its cage and monitor breathing and behavior for 5~10 minutes.</li>
</ol>

IV. In Vivo Imaging
We use the Caliper Life Sciences to monitor the behavior of cells injected into intrabursal cavity. Experiments using this system typically have a timeframe of 4~16 weeks from the time of tumor implantation.
<ol>
<li>	Prepare the solution of D-luciferin (substrate of firefly luciferase) by dissolving 5~20 mg in 1 mL PBS and filtering through 0.22 &mu;m membrane for sterilization.</li>
<li>	Charge the induction chamber by turning on both the oxygen and the isoflurane gas. Turn ON the gas flow to the induction chamber only. The isoflurane flow rate is maintained at a low level until animals are ready to be imaged.</li>
<li>	Check the animals' identification number and observable health. Place the animal in the induction chamber charged with isoflurane gas.</li>
<li>	Remove the animal from the chamber when the animal appears to be anesthetized. Deliver 200 &mu;L of prepared luciferin solution via i.p. injection using 30 G needle. It is important to record the time of injection in order to keep the time consistent between luciferin injection and imaging performance throughout the study.</li>
<li>	Place the luciferin-injected animal back into the induction chamber.</li>
<li>	Set the imaging system to the appropriate settings. Be sure to initialize the system before acquiring the first animal image.</li>
<li>	Turn OFF the gas flow to the induction chamber and turn ON the gas flow to the imaging chamber.</li>
<li>	Place the anesthetized animal dorsal or ventral side up. Be sure to place the animals' nose in a nose cone to maintain proper anesthesia induction. Make sure the animal is within the "point of interest grid" as indicated by green illumination.</li>
<li>	Close the door of the chamber and acquire the image at the appropriate time. Time can be determined by kinetics.</li>
<li>	Remove the animal from the imaging chamber and place it back into its cage. Monitor the animals' recovery as described in "Intrabursal Injection".</li>
</ol>

V. Representative Results
<img src="/files/ftp_upload/2125/2125fig1.jpg" alt="Figure 1" /> Figure 1. In Vivo imaging of ovarian tumor cells in an orthotopic mouse model. OVCAR5 cells expressing luciferase were injected intrabursally into right ovary and imaged over time. Images were taken 13 (left), 17 (middle), and 22 (right) days after the injection using the IVIS Spectrum imaging system. Dorsal side is shown in upper panel and ventral side is in lower panel. Note that the peritoneal spread of tumor cells 22 days following injection.
Experiments on animals were performed in accordance with the guidelines and regulations set forth by Fox Chase Cancer Center's Institutional Animal Care and Use Committee.

<ol>
	<li>Jemal, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cancer+statistics.">Cancer statistics.</a> CA Cancer J Clin. 59, 225-249 (2009).</li><li>Lynch, H. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Hereditary+ovarian+carcinoma:+heterogeneity,+molecular+genetics,+pathology,+and+management.">Hereditary ovarian carcinoma: heterogeneity, molecular genetics, pathology, and management.</a> Mol Oncol. 3, 97-137 (2009).</li><li>Yap, T. A., Carden, C. P., Kaye, S. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Beyond+chemotherapy:+targeted+therapies+in+ovarian+cancer.">Beyond chemotherapy: targeted therapies in ovarian cancer.</a> Nat Rev Cancer. 9, 167-181 (2009).</li><li>Killion, J. J., Radinsky, R., Fidler, I. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Orthotopic+models+are+necessary+to+predict+therapy+of+transplantable+tumors+in+mice.">Orthotopic models are necessary to predict therapy of transplantable tumors in mice.</a> Cancer Metastasis Rev. 17, 279-284 (1998).</li><li>Bibby, M. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Orthotopic+models+of+cancer+for+preclinical+drug+evaluation:+advantages+and+disadvantages.">Orthotopic models of cancer for preclinical drug evaluation: advantages and disadvantages.</a> Eur J Cancer. 40, 852-857 (2004).</li><li>Shaw, T. J., Senterman, M. K., Dawson, K., Crane, C. A., Vanderhyden, B. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Characterization+of+intraperitoneal,+orthotopic,+and+metastatic+xenograft+models+of+human+ovarian+cancer.">Characterization of intraperitoneal, orthotopic, and metastatic xenograft models of human ovarian cancer.</a> Mol Ther. 10, 1032-1042 (2004).</li><li>Greenaway, J., Moorehead, R., Shaw, P., Petrik, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Epithelial-stromal+interaction+increases+cell+proliferation,+survival+and+tumorigenicity+in+a+mouse+model+of+human+epithelial+ovarian+cancer.">Epithelial-stromal interaction increases cell proliferation, survival and tumorigenicity in a mouse model of human epithelial ovarian cancer.</a> Gynecol Oncol. 108, 385-394 (2008).</li><li>Connolly, D. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Animal+models+of+ovarian+cancer.">Animal models of ovarian cancer.</a> Cancer Treat Res. 149, 353-391 (2009).</li><li>Sadikot, R. T., Blackwell, T. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Bioluminescence+imaging.">Bioluminescence imaging.</a> Proc Am Thorac Soc. 2, 537-540 (2005).</li><li>Lehmann, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Longitudinal+and+multimodal+in+vivo+imaging+of+tumor+hypoxia+and+its+downstream+molecular+events.">Longitudinal and multimodal in vivo imaging of tumor hypoxia and its downstream molecular events.</a> Proc Natl Acad Sci U S A. 106, 14004-14009 (2009).</li><li>Connolly, D. C., Hensley, H. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Xenograft+and+Transgenic+Mouse+Models+of+Epithelial+Ovarian+Cancer+and+Non-Invasive+Imaging+Modalities+to+Monitor+Ovarian+Tumor+Growth+In+Situ:+Applications+in+Evaluating+Novel+Therapeutic+Agents.">Xenograft and Transgenic Mouse Models of Epithelial Ovarian Cancer and Non-Invasive Imaging Modalities to Monitor Ovarian Tumor Growth In Situ: Applications in Evaluating Novel Therapeutic Agents.</a> Current Protocols in Pharmacoogy. 45, (2009).</li></ol>

No conflicts of interest declared.

Ovarian cancer is the leading cause of death among all gynecologic malignancies 1. The high mortality rate of this disease is largely due to its late diagnosis and the lack of reliable diagnostic methods 2. Furthermore, conventional chemotherapy often encounters chemoresistance and relapse of cancer 3. Therefore, novel therapeutics is required to effectively target this disease. In development of new therapy targeting human ovarian cancer, it is critical to develop a representative animal model.

An orthotopic animal model has advantages over conventional xenograft models (e.g. subcutaneous or intraperitoneal injections of tumor cells) in that 1) it reproduces the primary site of tumor formation, 2) it represents common site of metastases, and 3) it provides tumor cells to interact with appropriate microenvironment 4, 5, 6, 7, 8. Rodents have a unique bursal membrane that surrounds the ovary and is continuous with the oviduct. This unique anatomy of rodents allows injection of ovarian tumor cells orthotopically. Intrabursally injected ovarian tumor cells behave similar to human disease, thereby growing within intrabursal membrane and spreading into peritoneal cavity as tumor progresses. Injection of cells stably expressing luciferases or fluorescent proteins also allows tracking behavior of tumor cells in real time. Bioluminescent and/or fluorescent imaging technology makes it possible to repeatedly image tumor cells over an extended period of time and study tumor growth, distribution, and regression in non-invasive manner 9, 10, 11.

In establishing the orthotopic model, it is critical to quickly remove the needle from the bursa upon injection. Abrupt removal of the needle seals the puncture site and prevents the leakage of injected cells. However, at the same time, the movement should be gentle not to tear the bursa. If leakage occurs during injection, it can cause cells to seed in the abdomen and potentially confound the study, i.e., premature spreading outside the ovary. In this event, the specific animal should be recorded and followed for the development of multiple tumor sites in the peritoneum prior to treatment or alternatively eliminated from the subsequent analyses. Prior to performing oral gavage, it is critical to check the length of the gavage tube by measuring from the tip of the animal's head to the last rib. It is helpful to mark the tube at the animal's nose and do not pass the tube past this mark. Insertion of the tube past this mark can result in a perforation to the stomach. Determining the length of the tube is especially important with younger animals or animals weighing under 20 g. Upon insertion of the gavage needle down the esophagus, there should be no resistance or struggle from the animal. It is important not to administer the solution or suspension too fast as this can lead to reflux and subsequently deliver inaccurate dose volume, as well as adding stress to the animal. For comparable imaging results from time to time, it is desirable to keep the time consistent between injection of luciferase substrate and imaging. The time lapse can be determined by taking series of images after substrate injection and observe the kinetics of signals. Development of an orthotopic mouse model of ovarian cancer, oral delivery of drugs, and in vivo imaging are necessary techniques for better understanding of development and spread of ovarian cancer and assessing novel therapeutic regimens that may ultimately improve the outcome of patient with this deadly disease.

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<td>Ketamine Hydrochloride</td>
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in vivo imaging and therapeutic treatments in an orthotopic mouse model of ovarian cancer

Human cancer and response to therapy is better represented in orthotopic animal models. This paper describes the development of an orthotopic mouse model of ovarian cancer, treatment of cancer via oral delivery of drugs, and monitoring of tumor cell behavior in response to drug treatment in real time using in vivo imaging system. In this orthotopic model, ovarian tumor cells expressing luciferase are applied topically by injecting them directly into the mouse bursa where each ovary is enclosed. Upon injection of D-luciferin, a substrate of firefly luciferase, luciferase-expressing cells generate bioluminescence signals. This signal is detected by the in vivo imaging system and allows for a non-invasive means of monitoring tumor growth, distribution, and regression in individual animals. Drug administration via oral gavage allows for a maximum dosing volume of 10 mL/kg body weight to be delivered directly to the stomach and closely resembles delivery of drugs in clinical treatments. Therefore, techniques described here, development of an orthotopic mouse model of ovarian cancer, oral delivery of drugs, and in vivo imaging, are useful for better understanding of human ovarian cancer and treatment and will improve targeting this disease.

Watch this Scientific Journal Video about In vivo Imaging and Therapeutic Treatments in an Orthotopic Mouse Model of Ovarian Cancer at JoVE.com

In vivo Imaging and Therapeutic Treatments in an Orthotopic Mouse Model of Ovarian Cancer

Orthotopic animal models of ovarian cancer replicate better human disease and therefore enhance our understanding of cancer progression and tumor response to therapy. A mouse model receives an intrabursal injection of luciferase-expressing ovarian tumor cells. Treatment is administered via oral gavage. Tumor growth is monitored by in vivo imaging system.

In vivo Imaging and Therapeutic Treatments in an Orthotopic Mouse Model of Ovarian Cancer

Human cancer and response to therapy is better represented in orthotopic animal models.  This paper describes the development of an orthotopic mouse model ...

in-vivo-imaging-therapeutic-treatments-an-orthotopic-mouse-model

Nanyang Technological University

Research

JoVE Journal

Biology

33.1K Views.  Women's Cancer Program.  中文 

Video: In vivo Imaging and Therapeutic Treatments in an Orthotopic Mouse Model of Ovarian Cancer

Orthotopic Mouse Model of Colorectal Cancer

The traditional subcutaneous tumor model is less than ideal for studying colorectal cancer. Orthotopic mouse models of colorectal cancer, which feature cancer cells growing in their natural location, replicate human disease with high fidelity. Two techniques can be used to establish this model. Both techniques are similar and require mouse anesthesia and laparotomy for exposure of the cecum. One technique involves injection of a colorectal cancer cell suspension into the cecal wall. Cancer cells are first grown in culture, harvested when subconfluent and prepared as a single cell suspension. A small volume of cells is injected slowly to avoid leakage. The other technique involves transplantation of a piece of subcutaneous tumor onto the cecum. A mouse with a previously established subcutaneous colorectal tumor is euthanized and the tumor is removed using sterile technique. The tumor piece is divided into small pieces for transplantation to another mouse. Prior to transplantation, the cecal wall is lightly damaged to facilitate tumor cell infiltration. The time to developing primary tumors and liver metastases will vary depending on the technique, cell line, and mouse species used. This orthotopic mouse model is useful for studying the natural progression of colorectal cancer and testing new therapeutic agents against colorectal cancer.

Two techniques can be used to establish this model: injection of a cancer cell suspension into the cecal wall or transplantation of a piece of subcutaneous tumor onto the cecum. This model is useful for studying the natural progression of colorectal cancer and testing new therapeutic agents against colorectal cancer.

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Imaging In-Stent Restenosis: An Inexpensive, Reliable, and Rapid Preclinical Model

Preclinical models of restenosis are essential to unravel the pathophysiological processes that lead to in-stent restenosis and to optimize existing and future drug-eluting stents.
A variety of antibodies and transgenic and knockout strains are available in rats. Consequently, a model for in-stent restenosis in the rat would be convenient for pathobiological and pathophysiological studies. 
In this video, we present the full procedure and pit-falls of a rat stent model suitable for high throughput stent research. We will show the surgical procedure of stent deployment, and the assessment of in-stent restenosis using the most elegant technique of OCT (Optical Coherence Tomography). This technique provides high accuracy in assessing plaque CSAs (cross section areas) and correlates well with histological sections, which require special and time consuming embedding and sectioning techniques. OCT imaging further allows longitudinal monitoring of the development of in-stent restenosis within the same animal compared to one-time snapshots using histology.

This video demonstrates how to use a preclinical inexpensive and reliable model to study pathobiological and pathophysiological processes of in-stent restenosis development. Longitudinal in vivo monitoring using OCT (Optical Coherence Tomography) and analysis of OCT images are also demonstrated.

Preclinical models of restenosis are essential to unravel the pathophysiological processes that lead to in-stent restenosis and to optimize existing and ...

Imaging Protein-protein Interactions in vivo

Protein-protein interactions are a hallmark of all essential cellular processes. However, many of these interactions are transient, or energetically weak, preventing their identification and analysis through traditional biochemical methods such as co-immunoprecipitation. In this regard, the genetically encodable fluorescent proteins (GFP, RFP, etc.) and their associated overlapping fluorescence spectrum have revolutionized our ability to monitor weak interactions in vivo using F&ouml;rster resonance energy transfer (FRET)1-3. Here, we detail our use of a FRET-based proximity assay for monitoring receptor-receptor interactions on the endothelial cell surface.

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This protocol describes how to image protein-protein interactions using a FRET-based proximity assay.

Protein-protein interactions are a hallmark of all essential cellular processes. However, many of these interactions are transient, or energetically weak, ...

Quantitative Measurement of Invadopodia-mediated Extracellular Matrix Proteolysis in Single and Multicellular Contexts

Cellular invasion into local tissues is a process important in development and homeostasis. Malregulated invasion and subsequent cell movement is characteristic of multiple pathological processes, including inflammation, cardiovascular disease and tumor cell metastasis1. Focalized proteolytic degradation of extracellular matrix (ECM) components in the epithelial or endothelial basement membrane is a critical step in initiating cellular invasion. In tumor cells, extensive in vitro analysis has determined that ECM degradation is accomplished by ventral actin-rich membrane protrusive structures termed invadopodia2,3. Invadopodia form in close apposition to the ECM, where they moderate ECM breakdown through the action of matrix metalloproteinases (MMPs). The ability of tumor cells to form invadopodia directly correlates with the ability to invade into local stroma and associated vascular components3. 
Visualization of invadopodia-mediated ECM degradation of cells by fluorescent microscopy using dye-labeled matrix proteins coated onto glass coverslips has emerged as the most prevalent technique for evaluating the degree of matrix proteolysis and cellular invasive potential4,5. Here we describe a version of the standard method for generating fluorescently-labeled glass coverslips utilizing a commercially available Oregon Green-488 gelatin conjugate. This method is easily scaled to rapidly produce large numbers of coated coverslips. We show some of the common microscopic artifacts that are often encountered during this procedure and how these can be avoided. Finally, we describe standardized methods using readily available computer software to allow quantification of labeled gelatin matrix degradation mediated by individual cells and by entire cellular populations. The described procedures provide the ability to accurately and reproducibly monitor invadopodia activity, and can also serve as a platform for evaluating the efficacy of modulating protein expression or testing of anti-invasive compounds on extracellular matrix degradation in single and multicellular settings.

We describe the prototypical method for producing microscope coverslips coated with fluorescent gelatin for visualizing invadopodia-mediated matrix degradation. Computational techniques using available software are presented for quantifying the resultant levels of matrix proteolysis by single cells within a mixed population and for multicellular groups encompassing entire microscopic fields.

Cellular invasion into local tissues is a process important in development and homeostasis.  Malregulated invasion and subsequent cell movement is ...

In Vivo 4-Dimensional Tracking of Hematopoietic Stem and Progenitor Cells in Adult Mouse Calvarial Bone Marrow

Through a delicate balance between quiescence and proliferation, self renewal and production of differentiated progeny, hematopoietic stem cells (HSCs) maintain the turnover of all mature blood cell lineages. The coordination of the complex signals leading to specific HSC fates relies upon the interaction between HSCs and the intricate bone marrow microenvironment, which is still poorly understood[1-2].
We describe how by combining a newly developed specimen holder for stable animal positioning with multi-step confocal and two-photon in vivo imaging techniques, it is possible to obtain high-resolution 3D stacks containing HSPCs and their surrounding niches and to monitor them over time through multi-point time-lapse imaging. High definition imaging allows detecting ex vivo labeled hematopoietic stem and progenitor cells (HSPCs) residing within the bone marrow. Moreover, multi-point time-lapse 3D imaging, obtained with faster acquisition settings, provides accurate information about HSPC movement and the reciprocal interactions between HSPCs and stroma cells.
Tracking of HSPCs in relation to GFP positive osteoblastic cells is shown as an exemplary application of this method. This technique can be utilized to track any appropriately labeled hematopoietic or stromal cell of interest within the mouse calvarium bone marrow space.

In Vivo 4-Dimensional Tracking of Hematopoietic Stem and Progenitor Cells in Adult Mouse Calvarial Bone Marrow

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In Vivo Microinjection and Electroporation of Mouse Testis

This article describes microinjection and electroporation of mouse testis in&#160;vivo as a&#160;transfection technique for testicular mouse cells to study unique processes of spermatogenesis. The presented protocol involves steps of glass capillary preparation, microinjection via the efferent duct, and transfection by electroporation.

This video and article contribution gives a comprehensive description of microinjection and electroporation of mouse testis in vivo. This particular ...

Validation of a Mouse Model to Disrupt LINC Complexes in a Cell-specific Manner

Nuclear migration and anchorage within developing and adult tissues relies heavily upon large macromolecular protein assemblies called LInkers of the Nucleoskeleton and Cytoskeleton (LINC complexes). These protein scaffolds span the nuclear envelope and connect the interior of the nucleus to components of the surrounding cytoplasmic cytoskeleton. LINC complexes consist of two evolutionary-conserved protein families, Sun proteins and Nesprins that harbor C-terminal molecular signature motifs called the SUN and KASH domains, respectively. Sun proteins are transmembrane proteins of the inner nuclear membrane whose N-terminal nucleoplasmic domain interacts with the nuclear lamina while their C-terminal SUN domains protrudes into the perinuclear space and interacts with the KASH domain of Nesprins. Canonical Nesprin isoforms have a variable sized N-terminus that projects into the cytoplasm and interacts with components of the cytoskeleton. This protocol describes the validation of a dominant-negative transgenic mouse strategy that disrupts endogenous SUN/KASH interactions in a cell-type specific manner. Our approach is based on the Cre/Lox system that bypasses many drawbacks such as perinatal lethality and cell nonautonomous phenotypes that are associated with germline models of LINC complex inactivation. For this reason, this model provides a useful tool to understand the role of LINC complexes during development and homeostasis in a wide array of tissues.

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Measuring the Stiffness of Ex Vivo Mouse Aortas Using Atomic Force Microscopy

We present detailed protocols for isolation of aortas from mouse and measurement of their elastic modulus using atomic force microscopy.

Arterial stiffening is a significant risk factor and biomarker for cardiovascular disease and a hallmark of aging. Atomic force microscopy (AFM) is a ...

Time-Resolved Fluorescence Imaging and Analysis of Cancer Cell Invasion in the 3D Spheroid Model

The invasion of cancer cells from the primary tumor into the adjacent healthy tissues is an early step in metastasis. Invasive cancer cells pose a major clinical challenge because no efficient method exist for their elimination once their dissemination is underway. A better understanding of the mechanisms regulating cancer cell invasion may lead to the development of novel potent therapies. Due to their physiological resemblance to tumors, spheroids embedded in collagen I have been extensively utilized by researchers to study the mechanisms governing cancer cell invasion into the extracellular matrix (ECM). However, this assay is limited by (1) a lack of control over the embedding of spheroids into the ECM; (2) high cost of collagen I and glass bottom dishes, (3) unreliable immunofluorescent labeling, due to the inefficient penetration of antibodies and fluorescent dyes and (4) time-consuming image processing and quantification of the data. To address these challenges, we optimized the three-dimensional (3D) spheroid protocol to image fluorescently labeled cancer cells embedded in collagen I, either using time-lapse videos or longitudinal imaging, and analyze cancer cell invasion. First, we describe the fabrication of a spheroid imaging device (SID) to embed spheroids reliably and in a minimal collagen I volume, reducing the assay cost. Next, we delineate the steps for robust fluorescence labeling of live and fixed spheroids. Finally, we offer an easy-to-use Fiji macro for image processing and data quantification. Altogether, this simple methodology provides a reliable and affordable platform to monitor cancer cell invasion in collagen I. Furthermore, this protocol can be easily modified to fit the users&#8217; needs.

Presented here is a protocol for the fabrication of a spheroid imaging device. This device enables dynamic or longitudinal fluorescence imaging of cancer cell spheroids. The protocol also offers a simple image processing procedure for the analysis of cancer cell invasion.

The invasion of cancer cells from the primary tumor into the adjacent healthy tissues is an early step in metastasis. Invasive cancer cells pose a major ...

In Vivo Two-photon Imaging of Megakaryocytes and Proplatelets in the Mouse Skull Bone Marrow

Platelets are produced by megakaryocytes, specialized cells located in the bone marrow. The possibility to image megakaryocytes in real time and their native environment was described more than 10 years ago and sheds new light on the process of platelet formation. Megakaryocytes extend elongated protrusions, called proplatelets, through the endothelial lining of sinusoid vessels. This paper presents a protocol to simultaneously image in real time fluorescently labeled megakaryocytes in the skull bone marrow and sinusoid vessels. This technique relies on a minor surgery that keeps the skull intact to limit inflammatory reactions. The mouse head is immobilized with a ring glued to the skull to prevent movements from breathing.
Using two-photon microscopy, megakaryocytes can be visualized for up to a few hours, enabling the observation of cell protrusions and proplatelets in the process of elongation inside sinusoid vessels. This allows the quantification of several parameters related to the morphology of the protrusions (width, length, presence of constriction areas) and their elongation behavior (velocity, regularity, or presence of pauses or retraction phases). This technique also allows simultaneous recording of circulating platelets in sinusoid vessels to determine platelet velocity and blood flow direction. This method is particularly useful to study the role of genes of interest in platelet formation using genetically modified mice and is also amenable to pharmacological testing (study the mechanisms, evaluating drugs in the treatment of platelet production disorders). It has become an invaluable tool, especially to complement in vitro studies as it is now known that in vivo and in vitro proplatelet formation rely on different mechanisms. It has been shown, for example, that in vitro microtubules are required for proplatelet elongation per se. However, in vivo, they rather serve as a scaffold, elongation being mainly promoted by blood flow forces.

In Vivo Two-photon Imaging of Megakaryocytes and Proplatelets in the Mouse Skull Bone Marrow

We describe here the method for imaging megakaryocytes and proplatelets in the marrow of the skull bone of living mice using two-photon microscopy.

Platelets are produced by megakaryocytes, specialized cells located in the bone marrow. The possibility to image megakaryocytes in real time and their ...