Method Article

Functional Assessment of Intestinal Permeability and Neutrophil Transepithelial Migration in Mice using a Standardized Intestinal Loop Model

DOI:

10.3791/62093

⸱

February 11th, 2021

 ,  , 
1Department of Pathology, University of Michigan, Ann Arbor

In This Article

Summary

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Dysregulated intestinal epithelial barrier function and immune responses are hallmarks of inflammatory bowel disease that remain poorly investigated due to a lack of physiological models. Here, we describe a mouse intestinal loop model that employs a well-vascularized and exteriorized bowel segment to study mucosal permeability and leukocyte recruitment in vivo.

Abstract

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The intestinal mucosa is lined by a single layer of epithelial cells that forms a dynamic barrier allowing paracellular transport of nutrients and water while preventing passage of luminal bacteria and exogenous substances. A breach of this layer results in increased permeability to luminal contents and recruitment of immune cells, both of which are hallmarks of pathologic states in the gut including inflammatory bowel disease (IBD).

Mechanisms regulating epithelial barrier function and transepithelial migration (TEpM) of polymorphonuclear neutrophils (PMN) are incompletely understood due to the lack of experimental in vivo methods allowing quantitative analyses. Here, we describe a robust murine experimental model that employs an exteriorized intestinal segment of either ileum or proximal colon. The exteriorized intestinal loop (iLoop) is fully vascularized and offers physiological advantages over ex vivo chamber-based approaches commonly used to study permeability and PMN migration across epithelial cell monolayers.

We demonstrate two applications of this model in detail: (1) quantitative measurement of intestinal permeability through detection of fluorescence-labeled dextrans in serum after intraluminal injection, (2) quantitative assessment of migrated PMN across the intestinal epithelium into the gut lumen after intraluminal introduction of chemoattractants. We demonstrate feasibility of this model and provide results utilizing the iLoop in mice lacking the epithelial tight junction-associated protein JAM-A compared to controls. JAM-A has been shown to regulate epithelial barrier function as well as PMN TEpM during inflammatory responses. Our results using the iLoop confirm previous studies and highlight the importance of JAM-A in regulation of intestinal permeability and PMN TEpM in vivo during homeostasis and disease.

The iLoop model provides a highly standardized method for reproducible in vivo studies of intestinal homeostasis and inflammation and will significantly enhance understanding of intestinal barrier function and mucosal inflammation in diseases such as IBD.

Introduction

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The intestinal mucosa encompasses a single layer of columnar intestinal epithelial cells (IECs), underlying lamina propria immune cells and the muscularis mucosae. Besides its role in the absorption of nutrients, the intestinal epithelium is a physical barrier that protects the body interior from luminal commensal bacteria, pathogens, and dietary antigens. In addition, IECs and lamina propria immune cells coordinate the immune response inducing either tolerance or response depending on the context and stimuli. It has been reported that the disruption of the epithelial barrier can precede the onset of pathologic mucosal inflammation and contribute to inflammatory bowel disease (IBD) encompassing both ulcerative colitis and Crohn's disease1,2,3,4,5,6,7. Individuals with ulcerative colitis present excessive transepithelial migration (TEpM) of polymorphonuclear neutrophils (PMN) forming crypt abscesses, a finding that has been associated with severity of disease8,9. Although compromised epithelial barrier function and excessive immune responses are hallmarks of IBD, there is a lack of experimental in vivo assays to perform quantitative assessments of intestinal permeability and immune cell recruitment into the intestinal mucosa.

The most common methods used to study intestinal epithelial permeability and PMN TEpM employ ex vivo chamber-based approaches using IEC monolayers cultured on semi-permeable porous membrane inserts10,11,12. The epithelial barrier integrity is monitored either by measurements of transepithelial electrical resistance (TEER) or the paracellular flux of the Fluorescein isothiocyanate (FITC)-labeled dextran from apical to basal compartment13,14,15. Similarly, PMN TEpM is typically studied in response to a chemoattractant that is added in the lower chamber16. PMN are placed in the upper chamber and after an incubation period, PMN that have migrated into the basal compartment are collected and quantified. While these methods are useful, easy to perform and very reproducible, they are obviously reductionist approaches and do not necessarily represent an accurate reflection of in vivo conditions.

In mice, a common assay to study intestinal paracellular permeability is by oral gavage of FITC-dextran and subsequent measurement of FITC-dextran appearance in the blood serum13,17. The disadvantage of this assay is that it represents an assessment of overall barrier integrity of the gastrointestinal tract rather than that of regional intestinal contributions. In addition, Evans blue is commonly used to evaluate vascular leakage in vivo18 and has also been employed to evaluate intestinal mucosal permeability in mouse and rat19,20,21. The quantification of Evans blue in the intestinal mucosa requires extraction from tissue employing incubation in formamide overnight. Therefore, the same tissue cannot be used to study intestinal epithelial permeability and neutrophil infiltration.

Here we highlight a simple protocol that reduces the number of animals needed to collect reproducible data on colonic mucosal permeability and leukocyte transepithelial migration in vivo. We, therefore, recommend the use of FITC-dextrans that are easily detectable in blood serum without compromising the integrity of intestinal loops which can be harvested for further analysis. Of note, the intestinal ligated loops have been used in various species (including mouse, rat, rabbit, calf) to study bacterial infection (such as Salmonella, Listeria monocytogenes and Escherichia coli)22,23,24,25 as well as intestinal permeability26; however, to the best of our knowledge there are no studies investigating mechanisms of PMN TEpM in specific regions in the intestine such as ileum or colon that are commonly involved in IBD.

Here we describe the mouse intestinal loop (iLoop) model that is a robust and reliable microsurgical in vivo method that employs a well-vascularized and exteriorized intestinal segment of either the ileum or proximal colon. The iLoop model is physiologically relevant and allows the assessment of intestinal barrier integrity and PMN TEpM on living mice under anesthesia. We demonstrate two applications: 1) quantification of serum levels of 4 kDa FITC-dextran after intraluminal administration in the iLoop 2) quantification of transmigrated PMN in the iLoop lumen after intraluminal injection of the potent chemottractant Leukotriene B4 (LTB4)27. Moreover, utilizing the iLoop model with Jam-a-null mice or mice harboring selective loss of JAM-A on IECs (Villin-cre;Jam-a fl/fl) compared to control mice, we are able to corroborate previous studies that have reported a major contribution for tight junction-associated protein JAM-A to intestinal permeability and neutrophil transmigration15,28,29,30,31.

The iLoop model is a highly functional and physiological method that can be used to corroborate in vitro assays. Furthermore, this is a versatile experimental model that allows the study of various reagents that can be injected into the loop lumen, including chemokines, cytokines, bacterial pathogens, toxins, antibodies and therapeutics.

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Protocol

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All animal experiments were conducted in accordance with the guidelines and policies of the National Institutes of Health and approved by the Institutional Animal Care & Use Committee at the University of Michigan.

1. Preoperative preparation

NOTE: This method was generated employing adult mice from C57BL/6 genetic background, aged 8 - 12 weeks. All mice were kept under strict specific pathogen free conditions with ad libitum access to normal chow and water. Results were obtained using C57BL/6, Jam-a - null mice (Jam-a-/-) or mice harboring selective loss of JAM-A on IECs (Villin-cre;Jam-afl/fl) and littermate Jam-afl/fl controls as previously described30.

  1. Area preparation
    1. Perform surgery in clean area. The intestinal Loop model, however, is a non-survival surgery that does not require aseptic/sterile technique. Observe veterinary sanitation practices and use cleaned surgical instruments (i.e., scrubbed with soap, rinsed with water followed by 70% ethanol).
    2. Turn on a temperature-controlled surgical board (or heating pads) and adapted light source to keep animal from hypothermia during the anesthesia and surgery.
    3. Prepare ligatures by cutting 6 cm segments of non-absorbable 4-0 silk surgical sutures.
    4. Prepare cotton gauzes (5 cm x 5 cm) that are cut in the center following an ellipsoid shape. These will be used to cover the midline laparotomy and prevent direct contact between the exteriorized iLoop and animal fur. Soak the cut gauzes in warm Hanks' Balanced Salt Solution (HBSS) in a petri dish container.
    5. Prepare wet cotton swabs soaked in warm HBSS that will be used to handle organs and exteriorized iLoop.
    6. Prepare 10 mL syringe filled with warm HBSS and attach to a yellow feeding tube. This syringe will be used for moisturizing exposed tissues during surgery and to gently flush the iLoop of fecal content.
  2. Animal preparation
    1. Anesthetize the animal in accordance with the approved animal protocol. In this protocol a mix of isoflurane and oxygen is administered through an anesthesia vaporizer. According to manufacturer's instructions, adjust oxygen flow rate to 1 L/min. Set the vaporizer to 5% and pre-charge the induction chamber. After 5 min, reduce isoflurane vaporizer to 2% - 2.5%.
    2. Place the animal in the induction chamber for 3 min - 5 min, then transfer animal to a heated surgery board and connect an anesthesia nosecone plug. Restrain the animal in supine position by the four limbs using adhesive tape.
      NOTE: As an anesthesia alternative, a mixture of ketamine (80 mg/kg - 100 mg/kg) and xylazine (5 mg/kg - 10 mg/kg) diluted in saline solution (0.9% NaCl) can be administrated by intraperitoneal injection. Anesthesia should be maintained throughout the surgery by intramuscular administration of ketamine/xylazine (at 0.1 - 0.25 times of initial doses) to ensure anesthetic depth. If available, an isoflurane anesthesia vaporizer is highly recommended to assure better reproducibility, survivability and prevent animal pain.
    3. Apply ophthalmic ointment to both eyes to prevent corneal desiccation.
    4. Perform a physical exam that includes heart rate (around 500 beats/min) and rhythm, mucous membrane color (pink), capillary refill time (< 2 s), respiratory rate (not lower than 40 - 60 breaths/min), and temperature (36.5 °C)32.
    5. Before proceeding to the next steps, assess anesthetic depth by pedal withdrawal reflex. Employ a painful stimulus (pinch) of the skin between the toes and/or toe pads. Mouse will respond by contracting and removing its leg. This pedal reflex disappears when animal is anesthetized deeply.
      ​NOTE: Monitoring of vitals and pedal reflex are recommended throughout anesthesia at minimum every 15 min. Institutional Animal Care and Use Committee (IACUC) guidelines for evaluation of anesthetic depth recommend monitoring of the following: (a) color of tail, foot and mucous membrane (such as tongue). Color pink as normal and pale or blue as indicative of decreased blood perfusion or respiratory distress; (b) evaluation of the breathing pattern as regular versus irregular breaths. A rectal temperature probe, rodent oximeter and heart rate monitors can be used for the assessment of body temperature, heart and respiratory rates, respectively.

2. Generation of the ileal loop

  1. Skin preparation: Scrub fur of the abdominal midline with alcohol swabs or gauze sponge soaked with 70% Ethanol. Do not wet a wide area of fur with alcohol to prevent hypothermia.
  2. Using scissors, perform a midline laparotomy. Make a vertical incision in the middle of the abdomen (about 2 cm in length) and expose the peritoneum. Be careful to not injure intra-abdominal organs.
  3. Place pre-cut wet cotton gauze over the exposed intra-abdominal cavity.
  4. Use wet cotton swabs to mobilize and exteriorize the caecum. Carefully place the caecum on the wet cotton gauze.
    NOTE: Caecum is localized in the left caudal quadrant of the abdominal cavity in a majority of mice independent of the sex of the animal.
  5. Use wet cotton swabs to mobilize and gently exteriorize the ileum of which the terminal section (distal end) is attached to the caecum (Figure 1B).
  6. Deploy at least 6 cm of terminal ileum on the wet cotton gauze without disruption of the mesenteric vessels and blood supply. Blood supply is maintained if there is no bleeding and the tissue maintains its pink color (Figure 1B).
    NOTE: Avoid drying of exposed tissues by maintaining tissues moist at all times with warm HBSS (every 2 - 3 min) using 10 mL syringe attached to a yellow feeding tube (step 1.1.6).
  7. Close to the caecum, identify the major artery supplying the ileum in the mesentery. Then locate two ligation sites in the mesentery that are free of critical blood vessels.
  8. Using blunt tissue forceps, firmly grab the terminal ileum (closest to the caecum) and using fine tip forceps, fenestrate the mesentery avoiding blood vessels. Place silk suture across the perforation and tie a surgical knot to create the first ligation (distal end of the loop).
  9. Use the ruler to measure 4 cm away from the first ligature and create the second ligature (proximal end of the loop) as mentioned in step 2.8 (Figure 1C).
  10. With fine scissors carefully cut next to each ligation to isolate the 4 cm ileal loop, keeping intact blood supply and mesenteric membrane.
    NOTE: Cut off both ends of the exteriorized segment of the iLoop, then flush gently as a necessary step that prevents interference with luminal contents (fecal matter), thus facilitating even dispersion of FITC-dextrans or chemotactic stimuli across the entire length of the isolated segment as well as allowing for more accurate quantification of leukocytes by flow cytometry. This procedure also allows uniform distension of the mucosa after injection of specified volumes of reagent and better reproducibility between animals.
  11. Gently flush the content of the ileal loop segment with warm HBSS using a flexible yellow feeding tube attached to a 10 mL syringe (see step 1.1.6).
  12. Ligate the two cut ends of the flushed ileal loop using silk suture.
  13. Use a 1 mL syringe with 30 G needle to slowly inject 250 µL of reagent such as FITC-dextrans (step 4.2) or chemokine (step 5.3) into the intestinal lumen. The ileal loop will inflate causing a moderate distension of the mucosa (Figure 1D).
    ​NOTE: Inject reagent into the loop lumen on the opposite side of the mesenteric artery. Be careful not to pull out the ileal loop from the animal while injecting to avoid tearing blood vessels and induce bleeding.
  14. Using wet cotton swabs, gently put back the ileal loop, proximal ileum and caecum.
  15. Use a needle holder, anatomical forceps and 3.0 non-absorbable silk sutures with reverse cutting needle to close the abdominal wall.
  16. Place the animal in a temperature-regulated anesthesia chamber for the incubation period.

3. Generation of the proximal colon loop (pcLoop)

NOTE: For details about mice that were used for the generation of the pcLoop, see the information provided at the beginning of the protocol section.

  1. Perform steps 2.1. - 2.4. as described above for the ileal loop.
  2. Using wet cotton swabs, exteriorize the entire ileum and place it on the top of a wet cotton gauze. Identify the proximal colon and the blood supply located in the mesocolon. Mobilize the proximal colon and by using fine tip forceps create the first ligature in an area free of vessels in the mesocolon at about 0.5 cm distal from the caecum (Figure 2B).
  3. Measure 2 cm from the first ligature and create a second ligature at an area free of blood supply in the mesocolon (Figure 2C).
  4. Using fine scissors carefully cut next to each ligation to isolate a 2 cm long pcLoop.
    NOTE: As mentioned in the note under step 2.10, it is important to cut off both ends to isolate a pcLoop that is gently cleaned of luminal contents. Carefully cut through the colonic tissue and mesocolon to prevent small vessels from bleeding into the intestinal lumen. If necessary, use thermal cautery to limit bleeding at the incision site.
  5. Gently flush the pcLoop with warm HBSS to remove feces using a flexible yellow feeding tube attached to 10 mL syringe (see step 1.1.6).
  6. Ligate the two cut ends of the flushed pcLoop using silk suture.
  7. Use a 1 mL syringe with 30G needle to slowly inject 200 μL of reagent such as FITC-dextrans (step 4.2) or chemokine (step 5.3) into the intestinal lumen. The pcLoop will inflate causing a moderate distension of the mucosa (Figure 2D).
    NOTE: Inject the reagent into the pcLoop lumen on the opposite side of the mesenteric artery. Ensure consistency between animals and create a 2 cm long pcLoop to ensure equal distension of the mucosa.
  8. Utilize wet cotton swabs to gently place back the ligated pcLoop, ileum and caecum into the abdominal cavity.
  9. Use a needle holder, anatomical forceps and 3.0 non-absorbable silk sutures with reverse cutting needle to close the abdominal wall.
  10. Place the animal in a temperature-regulated anesthesia chamber for the incubation period.

4. Quantitative assessment of intestinal permeability: 4 kDa FITC-dextran assay

  1. Perform an ileal loop or pcLoop (as described above).
  2. Using a 1 mL syringe with 30 G needle, inject into the intestinal lumen either 250 µL (ileum - step 2.13) or 200 µL (colon - step 3.7) of 4 kDa FITC-dextran solution (1 mg / mL in HBSS). Keep the unused FITC-dextran solution protected from light to prepare the standard curve after serum collection.
  3. For the ileal loop follow steps 2.14 to 2.16, for the pcLoop steps 3.8 to 3.10. Briefly, put organs and iLoop back in place into the abdominal cavity, close the abdominal wall.
  4. Place the animal for 120 min in a heated anesthesia chamber.
  5. After the incubation period open the abdominal wall, gain access to the heart and perform cardiac puncture using a 1 mL syringe with 25G needle to collect the blood. Transfer blood into a 1.3 mL serum clot activator tube, mix gently, and keep on ice protected from light. Collect at least 500 µL of blood per mouse.
    ​NOTE: Animals are euthanized when being under anesthesia by using a physical method such as decapitation or cervical dislocation, and in accordance with the approved animal protocol.
  6. Centrifuge serum clot activator tube for 5 min at 10,000 x g at room temperature according to manufacturer's recommendations. Collect the serum (supernatant) and transfer into a 1.7 mL centrifuge tube. Keep the tube on ice and protected from light.
  7. Quantification of fluorescence in blood serum
    1. Prepare a standard curve of FITC-dextran 4 kDa in serum of control mice (saline or HBSS is a valid alternative). Create a two-fold serial dilution with a starting concentration of 1 mg/mL FITC-dextran. FITC-dextran 4 kDa concentrations that are measured range between 0.25 mg/mL and 2 µg/mL.
    2. Transfer equal volume of the sample and standards to a black 96-well plate (flat bottom) and measure FITC in a fluorescence plate reader (Excitation 490 nm, Emission 520 nm), according to manufacturer's instructions and published protocols33. Calculate the FITC concentration based on the standard curve or present permeability values as fold-change normalized to the experimental control group.

5. Quantitative assessment of migrated PMN into the intestinal lumen after intraluminal stimulation with chemokines

NOTE: Very few PMN reside in the intestinal mucosa at the baseline level. Pretreatment of animals with pro-inflammatory cytokines results in an inflammatory environment that facilitates PMN recruitment from bloodstream into the intestinal mucosa.

  1. Using a 1 mL syringe with 30 G needle, perform intraperitoneal (i.p.) injection of a sterile solution of 100 ng of Tumor Necrosis Factor-α (TNFα) and 100 ng of Interferon-γ (INFγ) in 200 µL of Phosphate Buffered Saline (PBS).
  2. After 4 - 24 h of pretreatment with pro-inflammatory cytokines, perform an ileal loop or pcLoop (as described above).
  3. Using a 1 mL syringe with 30 G needle, inject into the intestinal lumen either 250 µL (ileum - step 2.13) or 200 µL (colon - step 3.7) of chemoattractant solution Leukotriene B4 (LTB4) 1 nM in HBSS.
    ​NOTE: Leukotriene B4 (LTB4) is used in this protocol as a potent chemoattractant for PMN. Other chemoattractants such as N-Formylmethionyl-leucyl-phenylalanine (fMLF) or chemokine (C-X-C motif) ligand 1 (CXCL1/KC) can also be used to induce significant recruitment of PMN into the colonic lumen30.
  4. For the ileal loop follow steps 2.14 to 2.16. For the pcLoop follow steps 3.8 to 3.10. Briefly, put organs and iLoop back in place into the abdominal cavity, close the abdominal wall.
  5. Place the animal for 60 min in a heated anesthesia chamber.
  6. Collection of the intestinal loop content
    1. Prepare solutions and store on ice: For the ileal loop and pcLoop, prepare a wash buffer containing 2 mM Ethylenediaminetetraacetic acid (EDTA), 5 mM Dithiothreitol (DTT) and 2% FBS in sterile PBS without calcium and magnesium.
    2. After the incubation period and under anesthesia maintenance, open the abdominal wall and pull out the iLoop (ileal loop or pcLoop). Euthanize animals when being under anesthesia by using a physical method such as decapitation or cervical dislocation, and in accordance with the approved animal protocol.
    3. Rinse loop with cold PBS to remove any residual blood contaminant and absorb excess of PBS with tissue wipes. Carefully collect the loop content into a 1.7 mL centrifuge tube (about 250 µL for ileal loop and 200 µL for pcLoop). Flush the loop with 500 µL cold wash buffer and, immediately after collection, place the tube on ice.
      ​NOTE: DTT helps to dissolve mucus. If iLoop luminal content is very viscous (depending on the mouse genetic background), dilute it 1:2 or 1:3 with wash buffer containing DTT.
    4. Pass the luminal content solution through a 35 µm nylon mesh filter using a 5 mL round-bottom tube with cell strainer cap. This step helps to remove tissue fragments and cell aggregates. Rinse the cell strainer with 1 mL of wash buffer.
    5. Centrifuge tube at 400 x g for 5 min at 4 °C. Discard supernatant, rinse pellet with 500 µL - 1 mL wash buffer, then centrifuge at 400 x g for 5 min, 4 °C.
    6. Resuspend iLoop luminal cell pellet in 200 µL of flow cytometry buffer (FCB) containing 2% FBS in sterile PBS without calcium and magnesium. Cells can be kept in a tube or transferred to a 96-well round bottom plate for flow cytometry staining and analysis.
  7. Flow Cytometry staining and analysis
    1. Compensation controls: white blood cells
      1. Prepare a 1 mL syringe with 25 G needle pre-filled with sterile 0.5 M EDTA (pH 8.0). 10% EDTA per expected blood volume (100 µL of EDTA for 1 mL blood).
      2. Collect blood under anesthesia by cardiac puncture. Transfer blood into a 1.7 mL tube, then centrifuge at 400 x g for 10 min, 4 °C.
        NOTE: While the mouse is under anesthesia use a physical method to confirm death in accordance with the approved animal protocol (such as cervical dislocation).
      3. Aspirate the supernatant. Resuspend the pellet in 1 mL of Ammonium-Chloride-Potassium (ACK) lysis buffer for the lysis of red blood cells. Incubate for 3 min - 5 min on ice. Centrifuge 400 x g for 5 min, 4 °C. If the pellet is still red, repeat this ACK lysis buffer step until pellet turns white.
      4. Resuspend the pellet in 1 mL FCB and plate 0.5 x 106- 1 x 106 of cells per well. Prepare five wells of a 96-well round-bottom plate. Place the plate on ice.
        ​NOTE: Use the same 96-well plate that contains the loop luminal contents (see step 5.6.6).
    2. Flow cytometry staining
      1. Centrifuge the 96-well plate for 5 min at 400 x g, 4 °C. Discard the supernatant and resuspend the pellets with 50 µL of Purified Rat Anti-Mouse CD16/CD32 as an Fc-Block (1 μg per 100 µL of FCB). Incubate for 5 min - 10 min on ice.
      2. Immunostaining of the iLoop luminal content: Prepare a mixture containing all fluorochrome-conjugated antibodies (1:50 dilution in FCB): anti-CD45-PerCP, anti-CD11b-PE and anti-Ly-6G-Alexa Fluor 647. Add 50 µL of the combination per well, for a final volume of 100 µL.
      3. Immunostaining of the white blood cells for compensations (1:50 dilution in FCB): Use 50 µL of FCB alone (unstained sample, well 1), 50 µL of each individual fluorochrome-conjugated antibody (wells 2 - 4), 50 µL of the combination of all fluorochrome-conjugated antibodies (well 5). Final volume of 100 µL.
      4. Incubate the plate for 30 min on ice protected from light.
      5. Centrifuge the plate for 5 min at 400 x g, 4 °C. Discard the supernatant and wash with 200 µL of FCB. Repeat this washing step twice.
      6. Add FCB 150 µL/well to the blood samples.
      7. Add 100 µL/well FCB to the iLoop luminal content sample. Then 50 µL/well of fluorescent counting beads.
    3. Flow cytometry analysis
      1. Gate for CD45 positive events and for the expression of Ly-6G-/Gr-1 and CD11b30.
      2. Use 100 µL of the sample volume as a stop condition.
      3. Calculate the absolute number of PMN that has migrated into the iLoop lumen following the information provided by the manufacturer of the fluorescent counting beads.
        NOTE: Data may be presented as (1) total number of PMN in the lumen30,34,35, (2) number of PMN per gram of tissue as well as (3) number of PMN per mm3 by using the formula for volume of a cylinder: V= π(pi) r 2 h (V for volume, r for radius and h for height).

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Results

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A schematic representation of the ileal loop and pcLoop models is depicted in Figure 1 and Figure 2, respectively. The anatomical pictures display the critical steps of the procedure including exteriorization of the intestinal segment (Figure 1B and Figure 2B), identification of an appropriate location for ligations that allows minimal disturbance of blood supply (

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Discussion

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The mechanisms responsible for dysregulation of intestinal barrier function and immune cell recruitment under pathologic conditions such as IBD are incompletely understood. Here, we detail a robust in vivo murine model that employs a well-vascularized exteriorized intestinal segment of either ileum or proximal colon and allows for assessment of intestinal permeability, neutrophil migration studies as well as other applications.

The iLoop is a non-recovery surgery that is performed on live anim...

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Disclosures

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The authors have nothing to disclose.

Acknowledgements

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The authors thank Dr. Sven Flemming of the University of Wuerzburg for his contributions to the establishment of the proximal colon loop model, Sean Watson for the management of the mouse colonies and Chithra K. Muraleedharan for helping with the acquisition of the pictures of the iLoop model. This work was supported by the German Research Foundation/DFG (BO 5776/2-1) to KB, R01DK079392, R01DK072564, and R01DK061379 to C.A.P.

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Materials

List of materials used in this article
NameCompanyCatalog NumberComments
Equipment and Material
BD Alcohol SwabsBD326895
BD PrecisionGlide Needle, 25G X 5/8"BD305122
BD PrecisionGlide Needle, 30G X 1/2"BD305106
BD 1ml Tuberculin Syringe Without NeedleBD309659
15ml Centrifuge TubeCorning14-959-53A
Corning 96-Well Solid Black Polystyrene MicroplateFisherScientific07-200-592
Corning Non-treated Culture Dish, 10cmMilliporeSigmaCLS430588
Cotton Tip Applicator (cotton swab), 6", sterileFisherScientific25806 2WC
Dynarex Cotton Filled Gauze Sponges, Non-Sterile, 2" x 2"Medex3249-1
EZ-7000 anesthesia vaporizer (Classic System, including heating units)E-Z SystemsEZ-7000
Falcon Centrifuge Tube 50ml VWR21008-940
Fisherbrand Colored Labeling TapeFisherScientific15-901-10R
Halsey Needle Holder (needle holder) FST12001-13
Kimwipes, small (tissue wipe)FisherScientific06-666
1.7ml Microcentrifuge Tubes Thomas Scientific c2170
Micro Tube 1.3ml Z (serum clot activator tube)Sarstedt 41.1501.105
Moria Fine ScissorsFST14370-22
5ml Polystyrene Round-Bottom Tube with Cell-Strainer Cap (35 µm nylon mesh)Falcon352235
Puralube Vet Ointment, Sterile Ocular LubricantDechra12920060
Ring Forceps (blunt tissue forceps)FST11103-09
Roboz Surgical 4-0 Silk Black Braided, 100 YDFisherScientificNC9452680
Semken Forceps (anatomical forceps)FST1108-13
Sofsilk Nonabsorbable Coated Black Suture Braided Silk Size 3-0, 18", Needle 19mm length 3/8 circle reverse cutting HenryScheinSS694
Student Fine Forceps, AngledFST91110-10
10ml Syringe PP/PE without needleMillipore Sigma Z248029
96 Well Cell Culture PlateCorning3799
Yellow Feeding Tubes for Rodents 20G x 30 mmInstechFTP-20-30
Solutions and Buffers
Accugene 0.5M EDTALonza51201
Ammonium-Chloride-Potassium (ACK) Lysing BufferBioWhittaker10-548E
Hanks' Balanced Salt SolutionCorning21-023-CV
Phosphate-Buffered Saline without Calcium and MagnesiumCorning21-040-CV
Reagents
Alexa Fluor 647 Anti-Mouse Ly-6G Antibody (1A8)BioLegend127610
CD11b Monoclonal Antibody, PE, eBioscience (M1/70)ThermoFisher12-0112-81
CountBright Absolute Counting BeadsInvitrogenC36950
DithiotreitolFisherScientificBP172-5
Fetal Bovine Serum, heat inactivatedR&D Systems511550
Fluorescein Isothiocyanate-Dextran, average molecular weight 4.000Sigma60842-46-8
IsofluraneHalocarbon12164-002-25
Leukotriene B4Millipore Sigma71160-24-2
PerCP Rat Anti-Mouse CD45 (30-F11)BD Pharmingen557235
Purified Rat Anti-Mouse CD16/CD32 (Mouse BD FC Block)BD Bioscience553142
Recombinant Murine IFN-γPeprotech315-05
Recombinant Murine TNF-αPeprotech315-01A

References

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  1. Olson, T. S., et al. The primary defect in experimental ileitis originates from a nonhematopoietic source. Journal of Experimental Medicine. 203 (3), 541-552 (2006).
  2. Jump, R. L., Levine, A. D. Mechanisms of natural tolerance in the intestine: implications for inflammatory bowel disease. Inflammatory Bowel Diseases. 10 (4), 462-478 (2004).
  3. Peeters, M., et al. Clustering of increased small intestinal permeability in families with Crohn's disease. Gastroenterology. 113 (3), 802-807 (1997).
  4. Michielan, A., D'Inca, R. Intestinal permeability in inflammatory bowel disease: Pathogenesis, clinical evaluation, and therapy of leaky gut. Mediators of Inflammation. 2015, 628157(2015).
  5. Chin, A. C., Parkos, C. A. Neutrophil transepithelial migration and epithelial barrier function in IBD: potential targets for inhibiting neutrophil trafficking. Annals of the New York Academy of Sciences. 1072, 276-287 (2006).
  6. Baumgart, D. C., Sandborn, W. J. Crohn's disease. Lancet. 380 (9853), 1590-1605 (2012).
  7. Ordás, I., Eckmann, L., Talamini, M., Baumgart, D. C., Sandborn, W. J. Ulcerative colitis. Lancet. 380 (9853), 1606-1619 (2012).
  8. Muthas, D., et al. Neutrophils in ulcerative colitis: A review of selected biomarkers and their potential therapeutic implications. Scandanavian Journal of Gastroenterology. 52 (2), 125-135 (2017).
  9. Pai, R. K., et al. The emerging role of histologic disease activity assessment in ulcerative colitis. Gastrointestinal Endoscopy. 88 (6), 887-898 (2018).
  10. Parkos, C. A., Delp, C., Arnaout, M. A., Madara, J. L. Neutrophil migration across a cultured intestinal epithelium. Dependence on a CD11b/CD18-mediated event and enhanced efficiency in physiological direction. The Journal of Clinical Investigation. 88 (5), 1605-1612 (1991).
  11. Brazil, J. C., Parkos, C. A. Pathobiology of neutrophil-epithelial interactions. Immunological Reviews. 273 (1), 94-111 (2016).
  12. Thomson, A., et al. The Ussing chamber system for measuring intestinal permeability in health and disease. BMC Gastroenterology. 19 (1), 98(2019).
  13. Li, B. R., et al. In vitro and in vivo approaches to determine intestinal epithelial cell permeability. Journal of Visualized Experiments. (140), e57032(2018).
  14. Srinivasan, B., et al. TEER measurement techniques for in vitro barrier model systems. Journal of Laboratory Automation. 20 (2), 107-126 (2015).
  15. Fan, S., et al. Role of JAM-A tyrosine phosphorylation in epithelial barrier dysfunction during intestinal inflammation. Molecular Biology of the Cell. 30 (5), 566-578 (2019).
  16. Parkos, C. A. Neutrophil-epithelial interactions: A double-edged sword. American Journal of Pathology. 186 (6), 1404-1416 (2016).
  17. Volynets, V., et al. Assessment of the intestinal barrier with five different permeability tests in healthy C57BL/6J and BALB/cJ mice. Digital Diseases and Sciences. 61 (3), 737-746 (2016).
  18. Wick, M. J., Harral, J. W., Loomis, Z. L., Dempsey, E. C. An optimized evans blue protocol to assess vascular leak in the mouse. Journal of Visualized Experiments. (139), e57037(2018).
  19. Tateishi, H., Mitsuyama, K., Toyonaga, A., Tomoyose, M., Tanikawa, K. Role of cytokines in experimental colitis: relation to intestinal permeability. Digestion. 58 (3), 271-281 (1997).
  20. Mei, Q., Diao, L., Xu, J. M., Liu, X. C., Jin, J. A protective effect of melatonin on intestinal permeability is induced by diclofenac via regulation of mitochondrial function in mice. Acta Pharmacologica Sinica. 32 (4), 495-502 (2011).
  21. Vargas Robles, H., et al. Analyzing Beneficial Effects of Nutritional Supplements on Intestinal Epithelial Barrier Functions During Experimental Colitis. Journal of Visualized Experiments. (119), e55095(2017).
  22. Arques, J. L., et al. Salmonella induces flagellin- and MyD88-dependent migration of bacteria-capturing dendritic cells into the gut lumen. Gastroenterology. 137 (2), 579-587 (2009).
  23. Coombes, B. K., et al. Analysis of the contribution of Salmonella pathogenicity islands 1 and 2 to enteric disease progression using a novel bovine ileal loop model and a murine model of infectious enterocolitis. Infection and Immunity. 73 (11), 7161-7169 (2005).
  24. Everest, P., et al. Evaluation of Salmonella typhimurium mutants in a model of experimental gastroenteritis. Infection and Immunity. 67 (6), 2815-2821 (1999).
  25. Pron, B., et al. Comprehensive study of the intestinal stage of listeriosis in a rat ligated ileal loop system. Infection and Immunity. 66 (2), 747-755 (1998).
  26. Clayburgh, D. R., et al. Epithelial myosin light chain kinase-dependent barrier dysfunction mediates T cell activation-induced diarrhea in vivo. The Journal of Clinical Investigation. 115 (10), 2702-2715 (2005).
  27. Palmblad, J., et al. Leukotriene B4 is a potent and stereospecific stimulator of neutrophil chemotaxis and adherence. Blood. 58 (3), 658-661 (1981).
  28. Mandell, K. J., Babbin, B. A., Nusrat, A., Parkos, C. A. Junctional adhesion molecule 1 regulates epithelial cell morphology through effects on beta1 integrins and Rap1 activity. The Journal of Biological Chemistry. 280 (12), 11665-11674 (2005).
  29. Laukoetter, M. G., et al. JAM-A regulates permeability and inflammation in the intestine in vivo. Journal of Experimental Medicine. 204 (13), 3067-3076 (2007).
  30. Flemming, S., Luissint, A. C., Nusrat, A., Parkos, C. A. Analysis of leukocyte transepithelial migration using an in vivo murine colonic loop model. Journal of Clinical Investigation Insight. 3 (20), (2018).
  31. Luissint, A. C., Nusrat, A., Parkos, C. A. JAM-related proteins in mucosal homeostasis and inflammation. Seminars in Immunopathology. 36 (2), 211-226 (2014).
  32. Cesarovic, N., et al. Isoflurane and sevoflurane provide equally effective anaesthesia in laboratory mice. Lab Animal. 44 (4), 329-336 (2010).
  33. JoVE Science Education Database. Introduction to the Microplate Reader. Journal of Visualized Experiments. , JoVE, Cambridge, MA. e5024(2020).
  34. Kelm, M., et al. Targeting epithelium-expressed sialyl Lewis glycans improves colonic mucosal wound healing and protects against colitis. Journal of Clinical Investigation Insight. 5 (12), (2020).
  35. Azcutia, V., et al. Neutrophil expressed CD47 regulates CD11b/CD18-dependent neutrophil transepithelial migration in the intestine in vivo. Mucosal Immunology. , (2020).
  36. Yu, Y. R., et al. A protocol for the comprehensive flow cytometric analysis of immune cells in normal and inflamed murine non-lymphoid tissues. PloS One. 11 (3), 0150606(2016).
  37. Bradfield, P. F., Nourshargh, S., Aurrand-Lions, M., Imhof, B. A. JAM family and related proteins in leukocyte migration (Vestweber series). Arteriosclerosis, Thrombosis, and Vascular Biology. 27 (10), 2104-2112 (2007).
  38. Ebnet, K. Junctional Adhesion Molecules (JAMs): Cell adhesion receptors with pleiotropic functions in cell physiology and development. Physiological Reviews. 97 (4), 1529-1554 (2017).
  39. Sorribas, M., et al. FXR modulates the gut-vascular barrier by regulating the entry sites for bacterial translocation in experimental cirrhosis. Journal of Hepatology. 71 (6), 1126-1140 (2019).
  40. Mazzucco, M. R., Vartanian, T., Linden, J. R. In vivo Blood-brain Barrier Permeability Assays Using Clostridium perfringens Epsilon Toxin. Bio-Protocol. 10 (15), 3709(2020).
  41. Kelly, J. R., et al. Breaking down the barriers: the gut microbiome, intestinal permeability and stress-related psychiatric disorders. Frontiers in Cellular Neuroscience. 9, 392(2015).
  42. Fiorentino, M., et al. Blood-brain barrier and intestinal epithelial barrier alterations in autism spectrum disorders. Molecular Autism. 7 (1), 49(2016).
  43. Kelm, M., et al. Regulation of neutrophil function by selective targeting of glycan epitopes expressed on the integrin CD11b/CD18. FASEB Journal : An Official Publication of the Federation of American Societies for Experimental Biology. 34 (2), 2326-2343 (2020).

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Intestinal PermeabilityNeutrophil MigrationIntestinal Loop ModelEpithelial BarrierTransepithelial MigrationTight JunctionsFITC Dextran AssayInflammatory Bowel DiseaseFlow CytometryJAM A Protein

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