Islet transplantation has recently emerged as an acceptable clinical modality for restoring normoglycemia in patients with type 1 diabetes mellitus (T1DM). The long-term survival and function of islet grafts is compromised by immune rejection–related factors. Downregulation of factors that mediate immune rejection using RNA interference holds promise for improving islet graft resistance to damaging factors after transplantation. Here, we used a dual-purpose therapy/imaging small interfering (si)RNA magnetic nanoparticle (MN) probe that targets β2 microglobulin (B2M), a key component of the major histocompatibility class I complex (MHC I). In addition to serving as a siRNA carrier, this MN-siB2M probe enables monitoring of graft persistence noninvasively using magnetic resonance imaging (MRI). Human islets labeled with these MNs before transplantation into B2M (null) NOD/scid mice showed significantly improved preservation of graft volume starting at 2 weeks, as determined by longitudinal MRI in an adoptive transfer model (P < 0.05). Furthermore, animals transplanted with MN-siB2M–labeled islets demonstrated a significant delay of up to 23.8 ± 4.8 days in diabetes onset after the adoptive transfer of T cells relative to 6.5 ± 4.5 days in controls. This study demonstrated that our approach could protect pancreatic islet grafts from immune rejection and could potentially be applied to allotransplantation and prevention of the autoimmune recurrence of T1DM in islet transplantation or endogenous islets.
Type 1 diabetes mellitus (T1DM) is characterized by the selective and progressive destruction of pancreatic β-cells, leading to insulin dependency and serious complications (1). Pancreatic allotransplantation offers superior glycemic control for T1DM patients and can prevent or even reverse secondary complications (2). However, this procedure is associated with significant mortality and morbidity (3). β-Cell replacement by islet transplantation provides a less invasive alternative T1DM treatment, with reduced antigen load, relative surgical simplicity, and low morbidity (4). Unfortunately, even with the success of the Edmonton immunosuppressive protocol, only 20% of patients remained insulin-independent 3 years after islet transplantation (5). Studies indicate that several factors influence the decrease in islet graft function (6). Among them are immunologic factors that play a critical role because they contribute to innate and adaptive immune rejection (7), recurrence of autoimmunity (8), and toxicity associated with immunosuppressive agents (9,10).
The potential for islet grafts to elicit allo- or xenoimmunogenic responses depends on their major histocompatibility complex (MHC) compatibility with the recipient HLA (11). Alloreactivity is significantly reduced In HLA-matched islet transplantation (12); however, limited sources of donor islets and extensive HLA polymorphisms restrict HLA-matched allotransplantation (13), prompting the search for alternative transplant sources.
One approach involves the use of xenografts (14), although significant immunologic barriers must be overcome before xenotransplantation becomes a reality in a clinical setting (15). As such, a T cell–mediated immune response occurring within weeks or even days of grafting causes irreversible β-cell damage (16). Major immune contributors to this damage include cytotoxic cluster of differentiation (CD)8+ T cells that recognize antigenic peptides in context with MHC class I molecules in allo- and xenografts (17,18). Reduction or downregulation of MHC class I protein expression using RNA interference (RNAi) (19) has shown some success in overcoming the limitations of immune rejection in cell-based therapies. The delivery of short hairpin RNA to HeLa cells resulted in a selective and permanent silencing of MHC class I by up to 90%, even under inflammatory conditions (20). MHC class I knockdown was effective in preventing antibody-mediated cell lysis and CD8+ T cell response (20). Lentivirus-mediated silencing of HLA in human 293 cells promoted resistance to killing by alloreactive T-effector cells (21) and showed enhancement in hematopoietic stem cell transplantation (22). Encouraged by these results, we sought to use RNAi to disturb MHC class I expression in human islet cells through the silencing of β2 microglobulin (B2M), a key component of MHC class I molecules, thereby reducing graft rejection in a model of xenotransplantation.
Because a safe and highly efficient delivery method is essential for the eventual clinical application of RNAi in islet grafts, we used magnetic nanoparticles (MNs) as a delivery vehicle for B2M small interfering (si)RNA into islet cells. This approach was selected rather than viral vector nucleotide delivery because it is not undermined by excessive inflammation (23) or the potential for oncogenicity (24). In addition to serving as a siRNA carrier, the MNs enable the monitoring of graft persistence noninvasively using magnetic resonance imaging (MRI) (25,26). Treatment of human islets with these dual-purpose therapeutic/imaging MNs before transplantation resulted in significantly improved survival of grafts and a delay in the onset of hyperglycemia after the adoptive transfer of T cells to animals with newly established xenografts. Our approach provides for protection of transplanted islet grafts and can be potentially extended for various transplantation and cell therapy applications.
RESEARCH DESIGN AND METHODS
Probe synthesis and characterization.
The synthesized probe consisted of magnetic dextran-coated iron oxide MNs labeled with Cy5.5 near-infrared optical dye and conjugated to siRNA at the dextran surface. First, we synthesized Cy5.5-labeled MNs, as previously reported (27). Briefly, a solution of monoactivated Cy5.5 succinimide ester (Amersham Biosciences, Piscataway, NJ) in 20 mmol/L sodium citrate and 0.15 mol/L NaCl was reacted with previously dialyzed immunopure, aminoderivatized dextran-coated iron oxide (pH 8.5) with constant agitation for 12 h at room temperature. The Cy5.5-labeled aminated iron oxide (MN-Cy5.5) was purified from unreacted dye using a Sephadex G-25, PD-10 column (Amersham Biosciences). MN-Cy5.5 was then conjugated to the heterobifunctional cross-linker N-succinimidyl 3-(2-pyridyldithio) propionate (SPDP; Pierce Biotechnology, Rockford, IL) by means of the N-hydroxy succinimide ester, followed by purification using a Sephadex G-25, PD-10 column in PBS/EDTA (pH 7.5). The number of SPDP molecules per crystal was determined based on the release of pyridine-2-thione at 343 nm (e = 8.08 × 103 mol/cm) after the addition of 35 mmol/L of the reducing agent, tris-(2-carboxyethyl) phosphine hydrochloride (TCEP, Thermo Fisher Scientific, Rockford, IL) in DMSO. A ratio of 16 SPDP molecules per nanoparticle was obtained. The size of the MNs was 34.26 ± 0.29 nm with a polydispersity index (PDI) of 0.22. The ζ potential at pH 7.00 was +16.8 ± 2.65 mV.
Double-stranded siRNA targeting human B2M (NM 004048.2) and scrambled (SCR) siRNA were synthesized by Dharmacon (Lafayette, CO). The siRNAs were modified to incorporate a thiol group on the 5′ end of the sense strand. The disulfide protecting groups on 5′-S-S- were deprotected using TCEP according to the manufacturer's instructions. The B2M-targeting and scrambled siRNA duplexes were then conjugated to MN-Cy5.5-SPDP through the 5′-sense thiol group. The siRNA was reacted overnight (4°C) with the previously activated MN-Cy5.5-SPDP product via the SPDP cross-linker in PBS/EDTA (pH 8), followed by purification using a Quick Spin Column G-50 Sephadex Column (Roche Applied Science, Indianapolis, IN; Supplementary Fig. 1).
The resulting B2M-targeting and scrambled probes, designated MN-siB2M and MN-siSCR, respectively, were purified using magnetic separation columns (Miltenyi Biotec, Inc., Auburn, CA). The amount of conjugated siRNA was assayed using agarose gel electrophoresis. The amount of siRNA dissociated from the nanoparticles was assessed under reducing conditions by pretreatment with 15 mmol/L TCEP for 30 min. siRNA standards, untreated probes, and probes treated with a reducing agent were applied to a 2% agarose gel in TBE buffer (Invitrogen, Carlsbad, CA) and run at 145 V for 1 h. The gel was stained with 0.5 μg/mL ethidium bromide (Sigma-Aldrich, St. Louis, MO) for 30 min, and visualized using a Molecular Imager FX scanner (Bio-Rad Laboratories, Hercules, CA). On average, the conjugation resulted in 1.8 pmol siRNA/μg Fe (Supplementary Fig. 2).
Human islet culture and islet treatment with probe.
Human islets were obtained from the Integrated Islet Distribution Program (IIDP Centers, National Institutes of Health and Juvenile Diabetes Research Foundation). The viability and purity of the islets exceeded 85%. On arrival at our facility, islets were cultured in 24-well nontreated plates (Nunc, Roskilde, Denmark) at 1,000 islet equivalents (IEQ)/well in CMRL 1066 medium (GIBCO, Grand Island, NY) supplemented with 10% FBS and 100 μg/mL penicillin-streptomycin.
To mimic activated conditions, the upregulation of MHC class I molecules was accomplished by stimulation of human islets with 50 ng/mL recombinant human interferon (IFN)-γ (R&D Systems, Minneapolis, MN) for 48 h (28). For labeling experiments, 1000 IEQ were incubated with MN-siB2M or MN-siSCR for 48 h in the IFN-γ–containing medium (25 μg Fe, 45 pmol siRNA, in 1 mL medium).
Splenocyte isolation and islet protein-stimulated enzyme-linked immunosorbent spot (ELISPOT).
For the islet protein-stimulated ELISPOT, total splenocytes isolated from NOD mice 4–6 weeks of age (The Jackson Laboratory, Bar Harbor, ME) were prestimulated by incubation with sonicated islet proteins (5 μg/mL) or phorbol 12-myristate 13-acetate (PMA, Sigma-Aldrich, St. Louis, MO, 50 ng/ml) for 7 days (29). No stimulator was added to the mock controls. The CD8+ T cells were isolated from each group with a CD8a+ T Cell Isolation Kit (Miltenyi Biotec, Inc., Auburn, CA). The purity of the CD8+ T cells was evaluated by fluorescence-activated cell sorter (FACS) with PE-labeled rat anti-mouse CD8 monoclonal antibody (BD Biosciences, Bedford, MA) and fluorescein isothiocyanate (FITC)–labeled anti-mouse CD3 monoclonal antibody (Cedarlane Laboratories, Hornby, ON, Canada). The separated CD8+ T cells were seeded at 2 × 105/well in ELISPOT plates and incubated with islet proteins for another 48 h. The release of IFN-γ was assessed by ELISPOT according to the manufacturer’s protocol (R&D Systems, Inc.). The results were expressed as spot counts/2 × 105 CD8+ T cells.
Islet transplantation and adoptive transfer of splenocytes for induction of immunorejection.
All animal experiments were performed in compliance with institutional guidelines and approved by the subcommittee on research animal care at Massachusetts General Hospital.
The recipients were 5-week-old B2M-deficient (null) NOD/scid mice (n = 22; The Jackson Laboratory). Diabetes was induced by intraperitoneal injection of streptozotocin (STZ; 200 mg/kg body weight; Sigma-Aldrich) freshly dissolved in Na citrate buffer (30). Diabetes was confirmed by weight loss, polyuria, and blood glucose levels higher than 250 mg/dL. MN-siB2M–labeled human pancreatic islets were implanted under the left kidney capsule (1,500 IEQ/kidney) of B2M (null) NOD/scid mice (n = 10). For the control group, the same number of MN-Cy5.5–labeled islets was transplanted under the left kidney capsule of B2M (null) NOD/scid mice (n = 10).
Normoglycemia was restored in all animals 2–3 days after transplantation. To induce immune rejection, 1 week after transplantation, 5 × 106 splenocytes isolated from 8-week-old NOD mice (The Jackson Laboratory) were adoptively transferred to experimental and control mice intravenously. Two 5-week-old B2M (null) NOD/scid mice transplanted with MN-siB2M–labeled human pancreatic islets did not receive the splenocyte injection and served as a “no adoptive transfer” control group.
In vivo optical imaging.
All animals were fed an alfalfa-free diet (TestDiet, Richmond, IN) 2 weeks before islet transplantation. In vivo optical imaging was performed using a whole-body animal imaging system (IVIS Spectrum, Caliper Life Sciences, Hopkinton, MA), equipped with 10 narrow-band excitation filters (30-nm bandwidth) and 18 narrow-band emission filters (20-nm bandwidth). The Cy5.5 signal from the recipient mice was collected at 640 nm excitation and 720 nm emission. To validate the origin of the Cy5.5 signal in the animals, three-dimensional (3D) reconstruction was performed using Living Image 4.2 software (Caliper Life Sciences, Hopkinton, MA).
In vivo MRI of transplanted human islet grafts.
In vivo MRI was done using a 9.4-T scanner with a Bruker Biospin Avance Console equipped with ParaVision 5.1 software on 1, 7, 14, 21, 27, 35, and 42 days after adoptive transfer. Imaging protocols consisted of T2-weighted spin echo, T2*-weighted gradient echo, and multislice multiecho T2 map. T2-weighted images were analyzed on a voxel-by-voxel basis by fitting the T2 measurements to a standard exponential decay curve, defined by the equation: [y = Aexp (−t/T2)] (31). We calculated graft volumes by counting the number of voxels in each slice of a region of interest (ROI) surrounding the graft and multiplying by voxel volume (0.05 mm3) using Marevisi 3.5 software (Institute for Biodiagnostics, National Research Council, Canada). To assess graft survival, blood glucose levels of experimental and control mice were monitored using a Acensia Contour Blood Glucose Monitoring System (Bayer Health Care, Tarrytown, NY) twice weekly starting before STZ injection and extending 6 weeks after adoptive transfer.
Histology and fluorescence microscopy
In vitro studies.
In vitro labeling of human islets with MN-siRNA probes was confirmed by histologic analysis. After incubation for 48 h with the probes, the islets were fixed in 4% formaldehyde, embedded in paraffin, sectioned, and stained with Prussian blue to identify the presence of iron in labeled islets. Briefly, sections were immersed in Prussian blue solution containing 5% potassium ferrocyanide (ACROS Organics, Fairlawn, NJ) and 5% hydrochloric acid (Aldrich, Milwaukee, WI) for 30 min and counterstained with nuclear fast red (Sigma-Aldrich).
For fluorescence microscopy, islet sections were incubated with mouse monoclonal antibody to dextran (1:100 dilution; Stemcell Technologies, Vancouver, BC, Canada) at 4°C overnight, followed by an FITC-labeled goat anti-mouse IgG secondary antibody (1:100 dilution, Invitrogen). After incubation, slides were mounted with a mounting medium containing DAPI (Vectashield, Vector Laboratories, Inc., Burlingame, CA). Images were acquired on a Nikon Eclipse 50i microscope using a SPOT 7.4 Slider RTKE CCD camera (Diagnostic Instruments, Sterling Heights, MI) and analyzed with iVision 4.015 software.
To demonstrate B2M downregulation after incubation with the probes, in vitro islets were treated as described above, and islet sections were incubated with rabbit polyclonal antibody to B2M (1:500 dilution; Abcam) at 4°C overnight, followed by incubation with fluorescein-labeled anti-rabbit IgG (H+L; 1:200 dilution, Vector Laboratories, Inc.). After incubation, slides were mounted with a medium containing DAPI, as described above.
In vivo studies.
Mice from the experimental and control group (n = 2) were killed 2 weeks after adoptive transfer. Their left kidneys were removed, embedded in paraffin, and cut into 5-µm sections. After antigen retrieval with Tris-EDTA buffer (pH 8.0) in the microwave oven for 10 min, tissue sections were blocked in 5% normal goat serum in PBS. For human insulin and mouse CD8+ T cells double-staining, sections were incubated with a guinea pig anti-human insulin primary antibody (1:200 dilution, Abcam) and rat anti-mouse CD8 monoclonal antibody (1:50 dilution, Abcam), followed by an FITC-labeled goat anti-guinea pig secondary IgG (1:100 dilution, Abcam) and Alexa Fluor 594 conjugated secondary goat anti-rat IgG (1:50 dilution, Invitrogen). For human insulin and B2M double-staining, the sections were stained with a guinea pig anti-human insulin primary antibody (1:200 dilution, Abcam) and rabbit anti-human B2M monoclonal primary antibody (1:100 dilution, Abcam), followed by an FITC-labeled goat anti-guinea pig secondary IgG (1:100 dilution, Abcam) and Texas red conjugated goat anti-rabbit secondary IgG (1:100 dilution, Santa Cruz Biotechnology, Santa Cruz, CA). All sections were mounted with a mounting medium containing DAPI and analyzed using fluorescence microscopy, as described above.
Data are presented as mean ± SD. Statistical comparisons between two groups were evaluated by Student t test and corrected by one-way ANOVA for multiple comparisons using GraphPad Prism 5 (GraphPad Software, Inc., La Jolla, CA). A value of P < 0.05 was considered to indicate statistical significance. A Mantel-Cox log-rank test was used to compare the percentage of animals that developed diabetes.
In vitro labeling of the islets and downregulation of B2M
Probe accumulation in human pancreatic islet cells.
For efficient downregulation of the target gene, B2M, it is necessary to ensure adequate intracellular accumulation of the probe. On the basis of our prior experience with islet labeling (25,27), we incubated human islets with control and experimental probes for 48 h. Fluorescence microscopy showing excellent colocalization of the Cy5.5 signal with anti-dextran staining provided direct evidence that both probes were taken up by islet cells (Fig. 1). Further support for the probe accumulation was obtained by staining islets with Prussian blue for iron (Supplementary Fig. 3). Tiny blue dots in the cytoplasm of the islet cells represent clusters of nanoparticles, as described previously (26).
MTT assay performed on labeled islets showed that the treatment with the probes did not have any significant effect on islet viability (Supplementary Fig. 4A). Glucose-stimulated insulin secretion and the glucose-stimulation index were not affected in all treatment groups (Supplementary Fig. 4B and C).
Silencing of B2M in vitro.
Silencing efficiency of the probes was evaluated after human islets were incubated with MN-siB2M or control MN-siSCR probe for 48 h. As revealed by real-time RT-PCR, the B2M mRNA expression in the islets incubated with the MN-siB2M probe was reduced by 37% relative to the control probe under basal conditions (Fig. 2A). The protein level was also decreased in MN-siB2M–treated islets, as shown by Western blot analysis (Fig. 2A). To mimic inflammatory conditions in vivo, islets were treated with human IFN-γ, which produced a threefold increase of B2M mRNA expression. In the islets treated with the MN-siB2M probe, B2M mRNA expression was reduced by 46% relative to controls under IFN-γ–stimulated conditions (Fig. 2B). The protein level of B2M under IFN-γ–stimulated conditions was also decreased in MN-siB2M–treated islets, as demonstrated by Western blot (Fig. 2B). Additional evidence for decreased protein expression was obtained with fluorescence microscopy that showed reduced levels of staining for B2M under these conditions (Fig. 2C).
Islet protein-stimulated ELISPOT was used to evaluate CD8+ T-cell responsiveness against islet proteins. T cells were purified, and their purity was confirmed by FACS analysis (Supplementary Fig. 5). Immune responsiveness of CD8+ T cells was determined by calculating the number of activated IFN-γ–producing CD8+ T cells treated with islet lysates. As shown in Fig. 2D, the number of CD8+ T cells activated after incubation with islet lysates obtained from MN-siB2M–treated islets was significantly less than the number of activated CD8+ T cells obtained after incubation with lysates from sham-treated islets or islets treated with the MN-siSCR probe (P < 0.05).
In vivo protection of islet grafts from T-cell challenge
Monitoring changes in graft volume after adoptive transfer by in vivo MRI.
As we have previously shown, MRI provides a reliable method for monitoring changes in graft volume over time (26,32). Here, we monitored the renal subcapsular islet grafts of experimental and control mice after the T-cell challenge, which was done 1 week after transplantation, when most of the initial graft loss had already occurred and the graft was relatively stabilized (data not shown) (26). As seen in Fig. 3, grafts could be identified on T2*-weighted MRIs as pockets of signal loss disrupting the contour of the left kidney at the transplantation site. To correlate our findings, we used an alternative in vivo imaging modality to perform whole-body optical imaging of the same animals. Bright signal detected in the Cy5.5 channel originated from the mouse kidney, as was confirmed by 3D reconstruction of optical images and by the presence of the graft under the kidney capsule as shown postmortem (Supplementary Fig. 6 and Supplementary Videos 1 and 2).
To compare the relative changes of graft volumes between experimental and control groups, we performed a semiquantitative ROI analysis of T2 maps. As expected, graft volumes of experimental and control mice decreased after adoptive transfer. However, the rate of decrease in the experimental group was significantly lower than in the control group. This difference was pronounced, starting at 2 weeks after adoptive transfer and continuing for the duration of the experiment (n = 6, P < 0.05; Fig. 4A).
We expected to observe a delay in hyperglycemia caused by the T-cell challenge as a consequence of the preserved graft volume. MN-siB2M–labeled and control islets were initially transplanted in STZ-induced diabetic animals and successfully restored normoglycemia, indicating that their function was preserved after labeling (Supplementary Fig. 7). After T cell adoptive transfer, we observed the increase in blood glucose levels in both groups (Supplementary Fig. 7). However, animals transplanted with MN-siB2M–labeled islets developed diabetes, determined as blood glucose >250 mg/dL on two consecutive measurements, significantly later than the control group. As evident from Kaplan-Meier analysis, diabetes developed at a mean of 6.5 ± 4.5 days in the control group but was delayed up to 23.8 ± 4.8 days in the experimental group (P = 0.0006, Fig. 4B). This study indicated that the protective effect of β2M silencing allowed for the delay in diabetes development and for longer function of the grafts.
In the “no adoptive transfer” control group (n = 2) transplanted with MN-siB2M–labeled islets, normoglycemia was restored 3 days after transplantation. Neither mouse redeveloped diabetes for the duration of the study, demonstrating that labeling with the probe was safe long-term.
Animals were killed two weeks after adoptive transfer, and their kidneys were processed for fluorescence microscopy. Staining of kidney sections for B2M showed markedly reduced protein expression in MN-siB2M–treated grafts compared with controls, indicating effective silencing of the gene (Fig. 5A). This was accompanied by a notably lower infiltration of MN-siB2M–treated islet grafts with CD8+ T cells compared with control grafts (Fig. 5B). Furthermore, Western blot analysis confirmed the reduction of B2M protein expression in the MN-siB2M–treated islet grafts compared with control grafts (Fig. 5C).
The major obstacle to successful islet transplantation is the potent T cell–mediated immune response occurring soon after the procedure that leads to β-cell damage (16). The interaction between MHC class I molecules and CD8+ T cells plays a major role in both allo- and xenograft rejection (33,34). MHC class I molecules are found on every nucleated cell of the body and consist of two components: the α chain (the heavy chain) and B2M (the light chain). The α chain and B2M are both essential for the proper folding of the entire MHC complex (35). Studies have shown that there is no detectable expression of MHC class I molecules on the surface of the cell in the absence of B2M (36).
We hypothesized that downregulation of B2M in pancreatic islet cells would lead to reduced recognition by T cells and, as a result, benefit the transplantation outcome. Therefore, the goal of our study was to downregulate B2M expression in human pancreatic islets before transplantation in B2M (null) NOD/scid mice using RNAi technology. We expected that aberrant expression of MHC class 1 proteins as the result of this downregulation would reduce or eliminate T cell recognition and provide the protection of pancreatic islet grafts in the xenotransplantation model used in this study. To deliver siRNA to intact pancreatic islets, we used MNs that serve the dual function of acting as a siRNA delivery vehicle while also providing information by MRI assessment about changes in graft volume over time in vivo.
To mimic immune rejection of the xenografts, we used an adoptive transfer model in which islet grafts were severely challenged by exposure to a sudden onslaught of primed T cells isolated from the spleen of immunocompetent mice (37). These cells caused immune rejection and were positively identified by histologic assessment (Fig. 5B) because B2M (null) NOD/scid mice lack endogenous CD8+ T cells (38). Previous studies showed that 50% of the islet xenografts were rejected 9 days after transplantation without immunosuppression, with a mean survival time of 10 ± 2.1 days (39). Downregulation of B2M expression in pancreatic islets led to significant protection of the grafts after adoptive transfer challenge. Diabetes development in this group occurred an average of 17 days later than in the control group. This was accompanied by a decline in graft volume in both groups, with the rate of this deterioration being significantly slower in the experimental group compared with the control group. MRI used in our study for estimation of graft volume is a modality with high spatial resolution, unlimited penetration through tissues, high tissue contrast, and tomographic capability. We have previously used it for the detection of graft reduction not only in the kidney capsule model of islet transplantation but also in a clinically approved model of islet grafting in the liver (25,26,31,32). Here, we demonstrate that in vivo MRI can serve as a tool for the determination of graft longevity during therapeutic intervention.
Clearly, our approach can potentially create a critical window of opportunity for the treatment of immune rejection and implementation of prompt intervention in a clinical scenario. Furthermore, it can be successfully applied to other situations where silencing MHC class I protein could be beneficial. For example, multiple studies have proven that this molecule also contributes to recurrence of autoimmune diabetes after islet transplantation in mice (40,41). The fact that B2M (null) NOD mice lacking CD8+ T cells do not develop insulitis implicates these cells as a crucial factor in the initiation of autoimmunity (42). Therefore, a B2M knockdown leading to targeted disruption of MHC class I molecule could potentially prevent autoimmunity in endogenous islets or autoimmune recurrence of TIDM in specific models of islet transplantation.
Immunosuppressive therapy can be toxic to transplanted islets and contribute to their progressive dysfunction (9,10). We believe that additional benefit from our current approach lies in the possibility of significantly reducing the dose of immunosuppressive therapy or ultimately avoiding the use of toxic immunosuppressants.
The major reason for the limited success of islet transplantation is a drastic decrease (up to 70%) of β-cell mass of the islet grafts during the first several weeks after transplantation (6,43); in fact, acute immune rejection begins as early as 1 week after transplantation. In our current study, we monitored the animals for 6 weeks after adoptive transfer, the period that most likely covered this initial damage. Our goal is to perform longitudinal studies in the future. In addition, we realize that despite B2M downregulation, the development of diabetes was not completely prevented but rather delayed. This is not unexpected, because factors other than infiltration of CD8+ T cells contribute to immune rejection, including involvement of antigen-presenting cells expressing MHC class II molecules (44) as well as CD4+ T cells (38), among others.
In addition, abolishing the recognition by CD8+ T cells could lead to the activation of natural killer (NK) cells, which recognize and eliminate abnormal cells (45) through the interaction between the NK group 2D (NKG2D) and ligands on target cells. In this particular study, we transferred splenocytes from NOD mice (Supplementary Fig. 8), whose NK cells had a functional deficiency (46) and therefore did not interfere with our observations. However, it should be possible to use our approach in the future to downregulate a variety of genes (including genes for NK cell ligands) responsible for islet damage by delivering a cocktail of nanoparticles or nanoparticles decorated with various sets of siRNAs.
In conclusion, to the best of our knowledge this is the first study that demonstrates the application of RNAi technology in combination with noninvasive imaging for the induction and detection of the delay in diabetes development caused by immune rejection in transplanted islets. We believe that this two-in-one theranostic approach could ultimately be applied in clinical settings for the protection of grafts in islet transplantation.
This study was supported by National Institutes of Health Grants 5R01DK-080784 and RO1DK-072137 to A.M.
No potential conflicts of interest relevant to this article were reported.
P.W. performed the in vitro experiments, animal surgery, and MRI scanning and participated in writing the manuscript. M.V.Y. synthesized the probe. C.R. assisted with optical imaging. A.R. and G.D. researched data. L.W. participated in animal studies. Z.M. participated in the experimental design. A.M. conceived the idea of the project and wrote the manuscript. A.M. is the guarantor of this work and, as such, had full access to all the data in the study and takes responsibility for the integrity of the data and the accuracy of the data analysis.
The authors thank Drs. James Markmann (Division of Transplantation, Department of Surgery, Massachusetts General Hospital) and Amol Kavishwar and Marytheresa Ifediba, MS (both from Molecular Imaging Laboratory, MGH/MIT/HMS Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital) for thoughtful discussions.
This article contains Supplementary Data online at http://diabetes.diabetesjournals.org/lookup/suppl/doi:10.2337/db12-0441/-/DC1.
See accompanying commentary, p. 3068.
- Received April 9, 2012.
- Accepted June 15, 2012.
- © 2012 by the American Diabetes Association.
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