Induction of Intestinal Graft-versus-host Disease and Its Mini-endoscopic Assessment in Live Mice

Podsumowanie

Here, we present a protocol that describes allogeneic hematopoietic stem cell transplantation and allows repetitive mini-endoscopic evaluations of the distal colon in situ for the presence, characteristics, and severity of colonic inflammation within live mice suffering from intestinal graft-versus-host disease.

Streszczenie

Acute graft-versus-host disease (GvHD) represents the most severe complication that patients previously undergoing allogeneic hematopoietic stem cell transplantation (allo-HCT) face and is frequently associated with a poor clinical outcome. While, for instance, GvHD manifestations of the skin are usually responsive to established immune-suppressive therapies and are, hence, not taking a fatal course, the presence and the intensity of intestinal GvHD, especially of the mid-to-lower parts of the gut, strongly influence the outcome and overall survival of patients with acute GvHD. Therapeutic options are essentially limited to the classic immune-suppressive agents yielding only moderate disease-mitigating effects. Hence, detailed knowledge about the tissue-resident immune cascade, changes in the intestinal microbiota, and the stromal response prior, upon, and after intestinal GvHD onset are urgently needed to understand the events and mechanisms underlying its pathogenesis and to develop innovative therapeutic options. Murine models of GvHD are frequently employed to identify and functionally assess molecules and pathways putatively driving intestinal GvHD. However, means to specifically monitor and evaluate intestinal inflammation over time are essentially lacking since established scores to assess and grade acute GvHD are routinely comprised of various parameters which rather reflect systemic GvHD manifestations. The detailed evaluation of intestinal GvHD has been restricted to studies using euthanized mice, thereby essentially excluding longitudinal (i.e., kinetic) analyses of the colonic compartment under a given experimental condition (e.g., antibody-mediated blockade of a proinflammatory cytokine) in live mice (i.e., in vivo). The mini-endoscopic in situ assessment of the distal colon of allo-HCT-treated mice described here allows a) a detailed macroscopic evaluation of different aspects of intestinal inflammation and b) the option to collect tissue samples for downstream analyses at various time points over the course of the observation period. Overall, the mini-endoscopic approach provides a major advance in preclinical noninvasive monitoring and assessment of intestinal GvHD.

Wprowadzenie

Hematopoietic malignancies directly arising from the hematopoietic stem cell compartment and uncontrolled, rapidly progressing, and severe immune-mediated disorders are often indications to perform allo-HCT^1,2. However, although accounting for the occurrence of the prognostic beneficial graft-versus-tumor response, donor lymphocytes are frequently inducing and promoting an unwanted immune-mediated attack of healthy tissue components within the allo-HCT recipient, a process that is called graft-versus-host disease³. Manifestations in the gut, the so-called intestinal GvHD, represent the most dreaded complication of acute GvHD, severe forms of which are routinely associated with a high mortality^1,2,4.

Overall, murine models of allo-HCT have emerged as invaluable tools to identify and study immune-mediated mechanisms underlying the pathogenesis of GvHD⁵. However, kinetic assessment of, for instance, beneficial effects of novel therapeutic interventions over time in live mice is routinely based on the determination of clinical GvHD scores⁶. While these scores are suitable to reflect, for instance, the overall disease burden (i.e., the systemic GvHD), clinical scores lack the sensitivity to reliably mirror organ-specific manifestations (e.g., in the gut). Hence, conclusions, for instance with respect to gut-protective effects of a given therapeutic intervention, that are based on these scoring systems usually fall short.

Despite major advances through the invention of novel whole-body imaging modalities in combination with the usage of either bioluminescent or fluorescent genetic mouse models^7,8, methodologies to directly and specifically assess the intestinal manifestation of GvHD in live mice are lacking. Hence, the rationale behind the protocol of the endoscopic assessment of the intestinal GvHD phenotype described in the next section is to overcome this obstacle. Furthermore, the motivation is also to reduce experimental mice numbers since, so far, a detailed assessment of the cellular, morphological, and molecular characteristics (e.g., by histopathology or molecular biology) of intestinal GvHD manifestation has ultimately required the sacrifice of the experimental mouse.

Our institution has previously reported on the methodology of a mini-endoscopic assessment of colonic manifestations in the course of syngeneic colitis models⁹. In the protocol presented here, we have refined and adapted the colonoscopic scoring matrix for alloresponse-driven colitis in live mice with intestinal GvHD upon transplantation of alloreactive HCT and donor lymphocytes in an MHC class I fully mismatched setting. We identified four parameters suitable to reflect intestinal GvHD-related colonic lesions. Furthermore, we established a system that allows a fine-tuned grading of any single determinant, resulting in a new score that readily informs the reader about the severity of intestinal GvHD present in a given mouse at a given time point. Histopathological analyses confirmed that an endoscopic score above a certain threshold is reliably predicting moderate-to-high grade tissue inflammation. Hence, mini-endoscopic evaluation appears to represent a working substitute for the gold standard histopathology that routinely requires the sacrifice of the experimental mice. Importantly, this protocol can be applied at virtually any given time point and can be repeatedly used during the course of the disease^10,11. Furthermore, in contrast to the usage of bioluminescence-dependent approaches, no labor-intense and time-consuming measures like intercrossing genetically modified mice are required and, hence, the methodology can be applied on virtually any mouse line of interest.

Taken together, given the detrimental clinical perspective of allo-HCT patients with severe intestinal GvHD, rapid scientific progress and more insight into the molecular mechanisms underlying the immune pathogenesis are urgently needed. Similarly, important, ethical considerations demand that the gain of knowledge should be achieved with the usage of the minimal number of experimental mice. Hence, both recognized claims on the research community exploring intestinal GvHD can be advanced by implementing serial mini-endoscopic evaluations of the colon in the experimental work chain to monitor and grade intestinal GvHD in live experimental mouse models, as described and validated in the protocol presented here.

Protokół

The experimental methods described here have been approved by the government of Mittelfranken, Bavaria, Germany.

1. GvHD induction

1. Day 0: Total body irradiation of the recipient mice
   1. Use female CD45.2⁺ H2kd⁺ BALB/c mice that are at least 10 weeks old as recipients.
   2. Weigh and record the weight of the recipient mice prior to GvHD induction.
      NOTE: Ensure that the recipient has a minimal body weight of 20 g. The starting body weight will serve as the reference value to calculate the weight loss of the individual mouse over the course of GvHD induction and progression.
   3. Place up to five mice in the container of the X-ray irradiator.
   4. Irradiate the mice by total body irradiation with a single dose of 8 Gy of X-ray. Use Cs¹³⁷ as a radiation source.
2. Day 1: Reconstitution of the irradiated mice with T-cell-depleted bone marrow
   NOTE: The transplantation of allogeneic bone marrow cells, as outlined and detailed under section 1.2, should take place within 24 h after irradiation. Perform the procedures described below in a sterile tissue culture hood and use filtered reagents. Use allogeneic CD45.1/Ly5.1 B6.SJL-Ptprca Pepcb/BoyCrl mice as donors for T-cell-depleted bone marrow.
   1. Euthanize CD45.1/Ly5.1 B6.SJL mice that will donate allogeneic bone marrow cells in accordance with the institutional guidelines, 12-24 h after the irradiation of the recipient BALB/c mice. For this, anesthetize the CD45.1/Ly5.1 B6.SJL mice by inhalation of 5% isoflurane. Continue with the isoflurane exposure over 1 min after breathing arrest and confirm euthanasia by cervical dislocation.
   2. Disinfect the fur and skin of the mouse thoroughly with 70% ethanol.
   3. Position the mouse onto a clean working sheath so that the mouse is in a prone position, with its hindquarters facing the experimenter. Lift the fur at the Achilles' heel with the tip of a Semken forceps with a length of 13 cm and serrated curved tips. Incise the skin between the forceps and the heel with hardened 8.5 cm fine scissors with straight tips.
   4. Elongate the incision cranially (i.e., from the heel over the lower leg and thigh to the hip region). Remove the skin and fur from the hind limb with the help of the forceps.
   5. Perform the same procedure on the other hind limb.
   6. Remove the hind limbs by cutting through the adjacent hip joints.
   7. Cut away the rear paws. Cut through the knee joint. Store the thigh and shank of every hind limb together in a 92 mm Petri dish filled with phosphate-buffered saline (PBS) solution on ice.
   8. Clean the femur and tibia bones carefully by removing as much muscle tissue as possible from every thigh and shank. Transfer the femur and tibia bones to a 50 mL tube filled with sterile RPMI 1640 medium and place it on wet ice until all tibia and femur bones collected in step 1.2.7 are cleaned from muscle tissue.
   9. To isolate the bone marrow, transfer one femur or tibia bone at a time (which has been cleaned as described in step 1.2.8) from the 50 mL tube to a Petri dish (with a diameter of 92 mm) filled with RPMI 1640 medium. Cut off the ends of the femur or tibia with a scalpel to get access to the cavity of the bone containing the bone marrow.
   10. Prepare a 50 mL collection tube with 5 mL of RPMI 1640 medium. Insert a 26 G needle attached to a 1 mL syringe filled with 1 mL of RPMI 1640 medium into the bone cavity and flush the bone marrow out of the cavity into the collection tube by pushing the plunger.
   11. Repeat step 1.2.10 until the bone appears light and shiny (i.e., the bone cavity is visibly devoid of reddish bone marrow). Discard the empty bone.
   12. Repeat steps 1.2.9 - 1.2.11, using all femur and tibia bones from step 1.2.8, and collect all recovered bone marrow pieces in the same 50 mL collection tube from step 1.2.10. Keep the collection tube on wet ice until all bones from step 1.2.8 have been processed accordingly.
   13. Create a single-cell suspension by softly pipetting the flushed, crumbly bone marrow pieces up and down. Filter the bone marrow single-cell suspension through a 40 µm mesh screen cell strainer placed on a new 50 mL collection tube.
   14. Centrifuge the 50 mL collection tube containing the bone marrow single-cell suspension at 450 x g for 5 min at 4 °C. Discard the supernatant.
   15. Resuspend the pellet in 5 mL of ACK lysing buffer (1 mM Na₂EDTA; 10 mM KHCO₃; 144 mM NH₄Cl; pH 7.2) for red blood cell lysis. Incubate the cell suspension for 3 min at room temperature. Afterward, immediately add 10 mL of PBS solution to the cell suspension.
   16. Centrifuge the suspension at 450 x g for 5 min at 4 °C. Discard the supernatant and resuspend the cells in 2 mL of PBS solution.
   17. Count the bone marrow cells, using a hemocytometer. Preserve an aliquot of 6 x 10⁶ cells for flow cytometry analysis to check the purity of the cells after cell purification (see step 1.2.20).
   18. For the depletion of T cells from the bone marrow single-cell suspension, use a commercially available cell purification kit. Magnetically deplete CD90.2⁺ cells (i.e., lymphocytes) from the total bone marrow cells, following the manufacturer's protocol.
   19. Count the T-cell-depleted bone marrow cells that have been isolated as described in step 1.2.18, using a hemocytometer. Preserve an aliquot of 1 x 10⁶ cells for flow cytometry analysis to be performed later on, as described in step 1.2.20.
       NOTE: The on-average cell yield derived from one donor mouse is usually from 2 x 10⁷ to 3.4 x 10⁷ T-cell-depleted bone marrow cells.
   20. Confirm a successful T-cell depletion by flow cytometry. Stain 1 x 10⁶ cells, preserved from steps 1.2.17 (bone marrow cells before magnetic cell separation) and 1.2.19 (T-cell-depleted bone marrow cells after magnetic cell separation), with the following antibodies: α-CD45.1 (A20), α-CD3 (17A2), α-CD4 (GK1.5), and α-CD8α (53-6.7). Use the remaining cells from step 1.2.17 as an unstained control and for single-staining controls, to set up the flow cytometer.
       1. Transfer 1 x 10⁶ cells from each sample to a well of a 96-well plate with a V-bottom to perform the flow cytometric staining procedure.
       2. Spin down the cells within the 96-well plate (step 1.2.20.1) at 450 x g for 5 min at 4 °C. Discard the supernatant and resuspend the cells in 100 µL of FACS buffer (PBS supplemented with 3% filtered bovine serum).
       3. Centrifuge the cells within the 96-well plate at 450 x g for 5 min at 4 °C. Discard the supernatant.
       4. Add an appropriate amount of the antibody of choice (compare with step 1.2.20) to the samples for single staining in 100 µL of FACS buffer.
       5. Prepare a mixture of all antibodies (master mix) containing the appropriate amounts sufficient to separately stain the bone marrow cell aliquots preserved from prior (see step 1.2.17) and after (see step 1.2.19) magnetic T-cell depletion. Add 100 µL of the master mix to both aliquots.
       6. Add only 100 µL of FACS buffer to the unstained sample.
       7. Incubate the cells within the 96-well plate for 20 min at 4 °C in the dark.
       8. Add 100 µL of FACS buffer and centrifuge the cells within the 96-well plate at 450 x g for 5 min at 4 °C. Discard the supernatant and resuspend the cells in 100 µL of FACS buffer.
       9. Centrifuge the cells at 450 x g for 5 min at 4 °C. Discard the supernatant and resuspend the cells in 250 µL of FACS buffer.
       10. Transfer the samples to a 5 mL polystyrene round-bottom tube and analyze them with a flow cytometer instrument that is able to detect the fluorescent molecules that were used to label the antibodies employed to characterize the cell samples (see step 1.2.20).
       11. Compare the cell composition from before and after the magnetic cell separation.
           NOTE: A purity of approximately 95% CD45.1⁺CD3^- (i.e., T-cell-depleted bone marrow) cells within the live gate is usually achieved.
   21. Wash the T-cell-depleted bone marrow cell suspensions 2x with PBS solution (450 x g for 5 min at 4 °C) and, finally, resuspend the cells in PBS solution, adjusting the cell concentration to 5 x 10⁷ cells/mL. Keep the cells on wet ice until the injection.
   22. Inject T-cell-depleted bone marrow cells into the recipient mice, which were irradiated the day before (see section 1.1).
       1. Place the experimental mouse in a leak-proof chamber and induce anesthesia by inhalation of up to 4% isoflurane, until the mouse is unconscious. Confirm analgesia and loss of consciousness by testing the loss of the righting reflex and the subsequent loss of the pedal withdraw reflex.
       2. Inject 5 x 10⁶ T-cell-depleted bone marrow cells (i.e., 100 µL of 5x10⁷ cells/mL) containing PBS solution using a 1mL syringe equipped with a 30 G needle intravenously into the retrobulbar space containing the venous sinus.
3. Day 2: Transfer of T cells
   NOTE: Perform the described procedures below in a sterile tissue culture hood and use filtered reagents. Use CD45.2 C57Bl/6 (wild-type; WT) mice as donors for alloreactive T cells. The usage of congenic marker systems allows the distinguishability between recipient (CD45.2⁺ H2kd⁺ Balb/c mice) and donor hematopoietic cell types (bone marrow cells: CD45.1⁺ H2kb⁺ B6.SJL mice; allogeneic T cells: CD45.2⁺ H2kb⁺ C57/Bl6 mice).
   1. Euthanize C57Bl/6 mice in accordance with the applying institutional guidelines and authorities. Therefore, anesthetize mice by inhalation with a concentration of 5% isoflurane. Continue the isoflurane exposure until 1 min after breathing arrest and confirm euthanasia by cervical dislocation. Disinfect the fur and skin of the mouse thoroughly with 70% ethanol.
   2. Place a strainer with a 40 µm mesh screen on a 50 mL collection tube. Remove the spleen and place it onto the strainer.
   3. With a syringe plunger, comminute the spleen in the strainer. Wash the strainer and syringe plunger with PBS to collect all splenocytes.
   4. Centrifuge the cells within the 50 mL collection tube at 450 x g for 5 min at 4 °C. Discard the supernatant.
   5. Resuspend the splenocytes in 3 mL of ACK lysing buffer to lyse red blood cells. Incubate the cell suspension for 3 min. Afterward, add 10 mL of PBS and centrifuge the cells at 450 x g for 5 min at 4 °C. Discard the supernatant and resuspend the splenocytes in PBS.
   6. Count the spleen cells, using a hemocytometer. Divert an aliquot of 6 x 10⁶ cells for flow cytometry analysis, to evaluate the magnitude of purification in step 1.3.9.
   7. For a total CD3⁺ T-cell isolation from total splenocytes, use a commercially available cell purification kit. Isolate the splenic T cells, following the manufacturer's protocol.
   8. Count the splenic CD3⁺ T cells isolated as described in step 1.3.7, using a hemocytometer. Preserve an aliquot of 1 x 10⁶ T cells for flow cytometry analysis.
      NOTE: The on-average yield of splenic T cells per donor mouse isolated by magnetic cell separation ranges from 1.3 x 10⁷ to 2 x 10⁷ cells.
   9. Confirm the success of the T-cell isolation by flow cytometry. For a detailed description of the staining protocol, confer and follow steps 1.2.20.1 - 1.2.20.10.
      1. Stain 1 x 10⁶ splenocytes of steps 1.3.6 (before the magnetic cell separation) and 1.3.8 (after magnetic cell separation) with the following antibodies: α-CD45.2 (104), α-CD3 (17A2), α-CD4 (GK1.5), and α-CD8α (53-6.7).
      2. Use the remaining cells from step 1.3.6 as an unstained control and for single staining with the respective antibodies, to set up the flow cytometer.
      3. Compare the cell composition before and after magnetic cell separation.
         NOTE: A purity of ≥95% of CD45.2⁺CD3⁺ T cells within the lymphocyte live gate should be accomplished.
   10. Wash the T cells 2x with PBS (450 x g for 5 min at 4 °C) and, finally, resuspend the cells in PBS solution, adjusting the cell concentration to 7 x 10⁶ cells/mL. Keep the cells on ice until the injection.
   11. Inject alloreactive, splenic T cells (see step 1.3.10) into irradiated BALB/c mice who have previously received CD45.1⁺ T-cell-depleted bone marrow cells (see step 1.2.22).
       1. Induce anesthesia by placing the experimental mouse in a leak-proof chamber in which it is exposed to up to 4% isoflurane until it loses its consciousness. Confirm analgesia and loss of consciousness by testing the loss of the righting reflex and the subsequent loss of the pedal withdraw reflex.
       2. Inject 0.7 x 10⁶ alloreactive CD3⁺ T cells using a 1 mL syringe equipped with a 30 G needle  (i.e., 100 µL of 7 x 10⁶ cells/mL) containing PBS solution (see step 1.3.10), intravenously into the retrobulbar space of the mice, to induce GvHD. Denominate these mice as the experimental group.
       3. Inject a different group of mice with 100 µL of PBS alone, intravenously into the retrobulbar space, and denominate this group as the control group, subsequently called "no-T-cell-transplanted (noT) mice".

2. Assessment of Systemic GvHD

NOTE: Perform this procedure in a semi-sterile surrounding in an experimental room licensed and equipped for handling live mice within the animal facility.

1. Follow the clinical course of GvHD in individual mice; specifically, assess and score the experimental mice 3x a week for the presence of clinical GvHD symptoms, based on a scoring system described below and adapted from a scoring system established previously by Cook et al.⁶.
   1. Weigh each mouse individually, record the weight, and calculate thespecific body weight loss in reference to the body weight that was determined prior to the start of the experiment (corresponding to 100%) on day 0 (step 1.1.2). Score a weight loss of less than 10% of the starting weight with grade 0, a weight loss between 10% and 25% with grade 1, and a weight loss of more than 25% with grade 3.
   2. Score the activity level of each mouse, discriminating mice with a normal activity level (score = 0) from mice with a moderately decreased activity level (score = 1) and mice with stationary behavior unless they are externally stimulated (score = 2).
   3. Score the fur texture, thereby discriminating a normal, shiny, and kempt fur (score = 0) from a moderately ruffled fur (score = 1) and the presence of bald spots (score = 2).
   4. Score the skin texture, discriminating normal skin (score = 0) from sporadic spots of scaling skin (e.g., at the tail and the paws) (score = 1) and obvious scaling and sore skin areas (score = 2).
   5. Analyze the consistency of secreted stool fractions. Score stool with a normal (i.e., hard consistency) with grade 0, stool with deformable and soft stool with grade 1, and stool without any consistency and, hence, with severe diarrhea with grade 2.
   6. Sum up all separately scored parameters to a maximal clinical score of 12 per mouse.
2. Consider and evaluate the criteria of ceasing the experiment due to the current disease severity level of the individual mouse, in accordance with the applying institutional guidelines and authorized animal protocol.

3. Assessment of Intestinal GvHD

1. Scoring of GvHD-related lesions by mini-endoscopy of the distal colorectal region
   NOTE: Perform this in a semisterile surrounding in an experimental room licensed and equipped for handling live mice within the animal facility. Use a mini-endoscopic workstation that is approved for the use of small animals.
   1. Prepare the endoscopic device by covering the telescope (with a diameter of 1.9 mm and a length of 10 cm) with the endoscopic examination sheath. Clean and sterilize the endoscope with water and ethanol.
   2. Switch on the computer, the adjustable xenon light source, and the camera module, and set the focus in a way that objects close to the lens give a clear image.
   3. Connect the air pump to the endoscopic sheath. To visualize the air stream, dip the tip of the endoscope into a beaker glass filled with water. Regulate the air stream by adjusting the valve between the air pump and the endoscopic sheath. Adjust it to a slow, constant air stream, reflected by a few continuously ascending bubbles.
   4. Place a mouse into a leak-proof chamber. Induce anesthesia by inhalation of up to 4% isoflurane until the mouse is unconscious. Confirm analgesia and an absent state of the reflexes by testing the loss of the righting reflex and the subsequent loss of the pedal withdraw reflex.
   5. Use an appropriate veterinary anesthesia machine in accordance with the animal protocol used. Transfer the mouse from the chamber to the colonoscopy workspace. Here, position the anesthetized mouse, with its nose in the nosecone (which is connected to the anesthesia instrument), onto a clean working sheath so that the mouse is in a prone position, facing the experimenter with its hindquarters.
   6. To maintain anesthesia during the colonoscopy procedure, reduce the isoflurane concentration to approximately 2%. Monitor the mouse's respiration and response to stimulation during the colonoscopy and adjust the isoflurane concentration at the vaporizer if needed. Cover the mouse's eyes with salve to prevent them from getting dry.
   7. Control the efficacy of the anesthesia by pinching between the toes of the mouse. In the case of absent reactivity, proceed to step 3.1.8.
   8. Lift the tail just above the tail root with one hand and carefully insert the endoscope, positioned in the other hand, via the anus into the rectum.
   9. While the air stream inflates the colorectal lumen, slowly and carefully move the endoscope forward in aboral direction.
   10. Place the endoscope in the middle of the colonic lumen and maintain this position in order to minimize contact with the colonic wall and to avoid making scratches, deeper wall-related injuries (e.g., resulting in bleeding), or even wall perforation (see step 3.1.17). Control this step by permanently watching the video stream (i.e., under constant visualization of the colonic compartment).
   11. If feces constrict the view, remove the endoscope and perform an enema by rectally flushing with up to 2 mL of saline, using a soft Pasteur pipette. Use as little liquid as possible, to prevent an unintended dilution of the feces and other secondary effects negatively affecting the characteristics of the mucosal surface and, ultimately, the scoring results.
   12. Try to regularly position the endoscope at a defined (i.e., distinct) anatomic site within the distal colon to standardize the scoring of colonic inflammation and to optimize the comparability of scoring results between mice and across experiments.
       NOTE: Normally, with the rigid endoscope, a maximal depth of 4 cm can be reached via the rectal route. Between 2 and 4 cm aborally, the colon regularly turns into a flexure that cannot be passed with the rigid colonoscope. Use the colon region distally adjacent to the flexure as the default scoring spot.
   13. Start to record the video stream and begin with the scoring of inflammation.
   14. Evaluate the GvHD-related inflammation of the colon by scoring the parameters explained and depicted in Table 1 and Figure 3.
       1. Move the endoscope at the scoring spot gently and slightly back- and forward to assess the different parameters.
       2. Assess the parameter "translucency", as well as the "stool consistency", by positioning the endoscope in a wider distance in relation to the colonic wall.
       3. Assess the parameters "granularity" and "vascularity" by positioning the endoscope in close proximity to the colonic wall. For this task, carefully apply well-dosed tension to the colonic wall with the tip of the endoscope.
   15. Upon completion of the scoring process, stop recording.
       NOTE: Afterward, the recorded video clip can be used in total or used to generate representative images (i.e., screenshots) of the mini-endoscopically assessed criteria overall contributing to colonic inflammation.
   16. Carefully remove the endoscope.
   17. Discontinue isoflurane exposition by transferring the mouse to a separate cage in which it is exposed to ambient air. Warm the mouse with a red-light lamp and observe the mouse until it recovers from the anesthetic and regains full consciousness.
       NOTE: Due to the air inflation of the colon during the endoscopy, the abdominal region of the mouse may appear puffed up directly afterward. While this is normal and of transient nature, prolonged signs of massive and even progressive inflation of the abdomen and failure of recovery of the mouse might indicate an unintended perforation of the colon (in this case, the mouse needs to be euthanized immediately).
   18. Upon complete recovery, place the mouse back into its respective cage.
   19. Optional approach: It is also possible to take view-guided tissue biopsies. Take the following steps.
       NOTE: The colonoscopy will be performed in the same way as described in steps 3.1.1 - 3.1.18, with the following modifications.
       1. In step 3.1.1, use an endoscopic examination sheath with a built-in working channel, instead of a simple examination sheath without working channels, for covering the telescope. Introduce a biopsy forceps into the working channel until its tip is just visible in front of the endoscope at the video screen because this largely prevents unintended injury to the intestine.
       2. Proceed with steps 3.1.2 - 3.1.11. Insert the endoscope into the colon and push it carefully forward to the spot of interest.
       3. Employ the help of a second experimenter for the task of taking colonic tissue biopsies. Ask the second experimenter to navigate the tip of the biopsy forceps to the colonic region of choice by pushing the forceps within the working channel slowly forward until the jaws of the forceps can be opened. Constantly watch the video stream during this procedure to minimize the risk of injuring the colonic wall.
       4. Recover a colonic wall tissue sample by carefully opening and closing the jaws of the biopsy forceps.
          NOTE: Do this with caution to prevent the perforation of the colonic wall. In the rare case of a colonic perforation, immediately sacrifice the affected mouse by applying measurements in accordance with the institutional guidelines and under the continuous administration of anesthetics.
       5. Pull back and remove the closed forceps out of the working channel. Remove the specimen from the jaws of the biopsy forceps by dipping and carefully shaking the opened forceps in sterile PBS solution. Afterward, choose proper storage conditions for the tissue sample, in accordance with the planned downstream analyses. After disinfection with 70% ethanol, the forceps might be reused to take further biopsies.
       6. After taking biopsies, remove the endoscope and finish the colonoscopy as described in steps 3.1.16 - 3.1.18.
2. Histopathological analysis
   1. Between days 26 and 30 after the X-ray irradiation, euthanize the allo-HCT recipient mice in accordance with applying institutional guidelines and authorities. For this, anesthetize the mice by inhalation of 5% isoflurane. Continue with the isoflurane exposure for 1 min after breathing arrest and confirm euthanasia by cervical dislocation. Thoroughly disinfect the fur and skin of the mouse with 70% ethanol.
   2. Open the abdominal cavity and remove the colon. Transfer it to a Petri dish (with a diameter of 92 mm) with PBS.
   3. Fill a 5 mL dispenser tip with PBS. With the help of a Semken forceps with a length of 13 cm and serrated curved tips, slip the distal part of the colon (approximately 5 mm) over the tip of the dispenser tip. Carefully fix the colon with the forceps at the dispenser tip and flush the colon with PBS by pressing down the plunger of the dispenser tip to remove feces from the intestine.
   4. Cut out a colonic segment located about 5 mm from the anus, with the help of a scalpel.
   5. Fix the resected gut specimen in 4.5% formaldehyde overnight. Before embedding it in paraffin, place the tissue in an upright position.
   6. Cut 3 µm cross sections of paraffin-embedded colon tissue and stain them with hematoxylin and eosin (HE), using standard staining protocols.
   7. Prepare HE-stained cross sections of colon tissue samples.
   8. Adapted from the scoring matrix reported by Kaplan et al.¹², histopathologically score the inflammatory activity semiquantitatively, with scores from 0-3: no inflammation (score = 0), mild inflammation (score = 1), moderate inflammation (score = 2), and severe inflammation (score = 3).
      NOTE: Ideally, employ for this task the expertise of a pathologist who is experienced in the evaluation of murine intestinal GvHD and blinded to the nature of the experimental and control groups.

Wyniki

The current protocol, describing the mini-endoscopic evaluation of intestinal GvHD-associated lesions of the distal colon, has been established and validated in mice previously subjected to the systemic induction of a severe acute GvHD model. In this study, we used an MHC class I fully mismatched model system in which BALB/c mice were lethally irradiated, followed by the transplantation of T-cell-depleted allogeneic bone marrow and by the administration of GvHD-inducing alloreactive C57BL...

Dyskusje

The protocol describes the methodology of induction and mini-endoscopic assessment of the colonic phenotype observed in the course of intestinal GvHD. It serves the wider purpose of enabling scientists to study intestinal GvHD longitudinally and noninvasively over the entire disease course (i.e., from the onset of colonic manifestation and progression until maximal disease activity).

However, there are some critical steps and important limitations inherent to the presented methodologies the ex...

Materiały

Name	Company	Catalog Number	Comments
BIOBEAM 2000 Gamma Irradiator	Gamma-Service Meical GmbH
Phosphate-buffered saline (PBS )	Sigma-Aldrich Co. LLC.	D8662-6x500ML
Semken Forceps (lenght: 13 cm; serrated, curved tips)	Fine Science Tools	11009-13
Hardened Fine Scissors (lenght: 8,5 cm; straight tips; cutting edge: 24 mm)	Fine Science Tools	14090-09
RPMI-1640 Medium	Sigma-Aldrich Co. LLC.	R8758-500ML
Hypodermic needle (26 G)	B. Braun Melsungen AG	4657683
1 mL syring	B. Braun Melsungen AG	9166017V
50 mL tube	Sarstedt Ag & Co.KG	62,547,254
Cell strainer with a 40 µm mesh screen	BD Falcon	352340
Ammonium chloride (NH4Cl)	Sigma-Aldrich Co. LLC.	11209	ingredient of ACK lysing buffer
Ethylenediaminetetraacetic acid disodium salt dihydrate (Na2EDTA)	Carl Roth GmbH & Co.KG	8043.2	ingredient of ACK lysing buffer
Potassium bicarbonate (KHCO3)	Merck KGaA	1,048,540,500	ingredient of ACK lysing buffer
CD90.2 MicroBeads, mouse	Miltenyi Biotec GmbH	130-049-101	magnet cell separation to isolate T cell-depleted bone marrow cells
Pan T Cell Isolation Kit II, mouse	Miltenyi Biotec GmbH	130-095-130	magnet cell separation to isolate splenic T cells
Alexa Fluor 700 anti-mouse CD45.2 Antibody (clone: 104; lot: B252126; RRID: AB_493731)	Biolegend	109822
Pacific Blue anti-mouse CD3 Antibody (clone: 17A2; lot: B227246; RRID: AB_493645)	Biolegend	100214
FITC anti-mouse CD4 Antibody (clone: GK1.5; lot: B225057; RRID: AB_312691)	Biolegend	100406
PE/Cy7 anti-mouse CD45.1 Antibody (clone: A20; lot: B217246; RRID: AB_1134168)	Biolegend	110730
APC/Cy7 anti-mouse CD8a Antibody (clone: 53-6.7, lot: B247008; RRID: AB_312753)	Biolegend	100714
Filtrated bovine serum	Pan Biotec	P40-47500	ingredient of FACS buffer
96-well polystyrene V-bottom plates	Greiner Bio-One	651201
Polystyrene Round-Bottom Tube (5 mL)	Falcon	352052
BD LSRFortessa II flow cytometer	BD Bioscience Co.
Insulin syringe with sterile interior (30 G)	BD	324826
Oxy Vet Oxymat 3	Eickemeyer		oxygen concentrator  for anesthesia
NarkoVet	Eickemeyer	213062
Plexiglass chamber	Eickemeyer	214620
Straight Forward Telescope	KARL STORZ SE &Co KG	64301 AA	part of the experimental setup for colonoscopy
Protection and Examination Sheath	KARL STORZ SE &Co KG	61029 C	part of the experimental setup for colonoscopy
Examination Sheath with working channel	KARL STORZ SE &Co KG	61029 D	part of the experimental setup for colonoscopy
Biopsy Forceps	KARL STORZ SE &Co KG	61071 ZJ	part of the experimental setup for colonoscopy
175 Watt SCB XenonLight Source	KARL STORZ SE &Co KG	20132120	part of the experimental setup for colonoscopy
Fiber Optic Light Cable	KARL STORZ SE &Co KG	495 NL	part of the experimental setup for colonoscopy
Image 1 S3 Camera Head	KARL STORZ SE &Co KG	22220030	part of the experimental setup for colonoscopy
Image 1 SCB Camera Control Unit	KARL STORZ SE &Co KG	22200020	part of the experimental setup for colonoscopy
LCD monitor	Olympus	OEV181H	part of the experimental setup for colonoscopy
Forane / Isofluran	AbbVie Inc.	B506
Formaldehyde solution 37 %	Carl Roth GmbH & Co.KG	7398.1
5.0 mL Dispenser tip	Eppendorf AG	30089456