FeCo/graphitic-carbon nanocrystals (FeCo/GC) are biocompatible, high-relaxivity, multi-functional nanoparticles. Macrophages represent important cellular imaging targets for assessing vascular inflammation. We evaluated FeCo/GC for vascular macrophage uptake and imaging in vivo using fluorescence and MRI.
Methods and Results
Hyperlipidemic and diabetic mice underwent carotid ligation to produce a macrophage-rich vascular lesion. In situ and ex vivo fluorescence imaging were performed at 48 hours after intravenous injection of FeCo/GC conjugated to Cy5.5 (n = 8, 8 nmol of Cy5.5/mouse). Significant fluorescence signal from FeCo/GC-Cy5.5 was present in the ligated left carotid arteries, but not in the control (non-ligated) right carotid arteries or sham-operated carotid arteries (p = 0.03 for ligated vs. non-ligated). Serial in vivo 3T MRI was performed at 48 and 72 hours after intravenous FeCo/GC (n = 6, 270 µg Fe/mouse). Significant T2* signal loss from FeCo/GC was seen in ligated left carotid arteries, not in non-ligated controls (p = 0.03). Immunofluorescence staining showed colocalization of FeCo/GC and macrophages in ligated carotid arteries.
Citation: Kosuge H, Sherlock SP, Kitagawa T, Terashima M, Barral JK, Nishimura DG, et al. (2011) FeCo/Graphite Nanocrystals for Multi-Modality Imaging of Experimental Vascular Inflammation. PLoS ONE 6(1): e14523. https://doi.org/10.1371/journal.pone.0014523
Editor: Stefan Kiechl, Innsbruck Medical University, Austria
Received: July 2, 2010; Accepted: December 16, 2010; Published: January 14, 2011
Copyright: © 2011 Kosuge et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by grants from the National Institutes of Health (R01-HL078678, nih.gov), the American Heart Association (0825272-F, heart.org), and Stanford Bio-X Interdisciplinary Initiatives Program (biox.stanford.edu), as well as MRI research support from GE Healthcare (gehealthcare.com). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: Drs. McConnell and Nishimura receive research support from GE Healthcare. Dr. McConnell is on a Scientific Advisory Board for Kowa, Inc. This does not alter the authors' adherence to all the PLoS ONE policies on sharing data and materials. The other authors have declared that no competing interests exist.
Inflammation is a major contributor to atherosclerosis, a leading cause of death worldwide –. Macrophages in the vessel wall have been associated with atherosclerotic plaque rupture and acute myocardial infarction –. Thus, imaging of vascular macrophages may be useful for characterizing plaque biological activity.
Cellular and molecular imaging of atherosclerosis and vascular inflammation has made significant progress, but remains challenging –. FeCo/graphitic-carbon nanocrystals (FeCo/GC) are composed of an iron-cobalt (FeCo) core with a graphitic-carbon shell . We have shown that the FeCo core provides higher relaxivity for MRI compared to other commercially available contrast agents, while the graphite shell enables biocompatibility and high optical absorbance in the near-infrared region for potential thermal therapy . We have also shown the potential of FeCo/GC for stem cell imaging in vitro as well as high-resolution vascular angiography in vivo , , but in vivo cellular imaging of FeCo/GC has not been studied.
The aim of the current study was to investigate FeCo/GC for in vivo macrophage uptake and imaging in a murine model of vascular inflammation. We show carotid artery macrophages take up FeCo/GC and can be imaged by in situ fluorescence and in vivo high-field MRI.
Fluorescence imaging of carotid arteries after administration of FeCo/GC
Both in situ and ex vivo fluorescence imaging at 48 hours showed high signal from the ligated left carotid arteries, confirming FeCo/GC uptake in the vascular lesions (Figure 1A; yellow arrows). In contrast, there was no significant FeCo/GC accumulation seen in the non-ligated right carotid arteries (Figure 1A, red arrows). Furthermore, sham operated mice did not show significant signal in either left or right carotid arteries (Figure 1B).
(A) Both in situ and ex vivo images at 48 hours after FeCo/GC-Cy5.5 injection showed enhanced fluorescence signal localized to the ligated left carotid artery (yellow arrows), but not to the contralateral non-ligated right carotid (red arrows). (B) Sham-operated mice showed no significant signal in either the left or right carotid arteries. (C) Quantitative analysis of both in situ and ex vivo fluorescence signal intensity showed significantly greater fluorescence from ligated left carotid arteries compared to non-ligated right carotid arteries. †p = 0.03 vs. right carotid, *p = 0.046 vs. sham left carotid.
Quantitative analysis of both in situ and ex vivo signal intensities showed that the ligated left carotid arteries had significantly higher fluorescence than the control (non-ligated) right carotid arteries (Figure 1C; in situ (left vs. right): 2.3±0.4 vs. 0.7±0.1, p = 0.03, ex vivo (left vs. right): 59.2±17.2 vs. 0.3±0.3, p = 0.03). Also, the ligated left carotids had significantly higher fluorescence than sham left carotids (in situ (ligated vs. sham): 2.3±0.4 vs. 0.9±0.1, p = 0.046, ex vivo (ligated vs. sham): 59.2±17.2 vs. 0.3±0.3, p = 0.046).
In vivo MRI of carotid arteries after administration of FeCo/GC
MRI prior to FeCo/GC administration (Figure 2A-Pre) showed that the ligated left carotid artery (yellow arrow), as expected, was smaller than the non-ligated right carotid artery (red arrow). Post FeCo/GC injection, serial MRI showed reduction in left carotid lumen area due to T2* signal loss from FeCo/GC accumulation at both 48 and 72 hours. In contrast, luminal area reduction due to T2* signal loss was not seen in the control (non-ligated) right carotid arteries (Figure 2A).
(A) The ligated left carotid artery (yellow arrow), as expected, was smaller than the non-ligated right carotid artery (red arrow) prior to FeCo/GC injection (Pre). After FeCo/GC injection, T2* signal loss of the ligated left carotid artery was seen at 48 and 72 hours. Luminal area reduction was not seen in the control (non-ligated) right carotid artery. (B) Quantitative analysis showed significant % reduction in lumen area of ligated left vs. non-ligated right carotid arteries. †p = 0.03 vs. Pre, *p = 0.03 vs. right carotid.
The measured % reduction of carotid lumen area at 48 and 72 hours for the ligated left carotid arteries was significantly greater than for the non-ligated controls, indicating the accumulation of FeCo/GC in the carotid lesion (Figure 2B; 48 hours (left vs. right): 60.1±10.7% vs. 16.9±9.9%, p = 0.03; 72 hours (left vs. right): 83.9±4.6% vs. 21.3±7.2%, p = 0.03). Furthermore, preliminary testing (n = 3) of an eight-fold lower FeCo/GC dose at higher field strength (7T) also showed T2*-induced lumen reduction in ligated left vs. right carotid arteries (28.0±5.7% vs. −5.56±1.2%, p = 0.1).
Immunohistochemistry for macrophages demonstrated that there was substantial macrophage infiltration in the neointima of ligated left carotid arteries, accounting for 18.9±1.9% of the neointimal area (Figure 3A,C). There was also significant smooth muscle cell proliferation, accounting for 34.5±3.7% of the neointimal area (Figure 3B,C). Furthermore, carotid immunofluorescence staining showed that FeCo/GC colocalized with macrophages (Figure 3D). The specificity of FeCo/GC for macrophages was further confirmed by immunofluorescence staining showing abundant uptake in the macrophage-rich liver and scant uptake in the macrophage-poor heart (Figure 3E,F).
(A) Immunohistochemical staining showed macrophages (by anti-Mac3 antibody) infiltrating the neointima of the ligated left carotid artery. (B) Immunohistochemical staining for smooth muscle cells (by anti-SMA antibody). (C) Quantitative analysis of proportion of neointima composed of macrophages and smooth muscle cells. (D) Immunofluorescent staining demonstrated macrophages (green), FeCo/GC-Cy5.5 (red), nuclei (blue), and combined staining with strong colocalization (yellow), particularly near the luminal border (arrow). (E) Immunofluorescent staining of the macrophage-rich liver also demonstrated strong colocalization (yellow) of FeCo/GC and macrophages. (F) By contrast, the macrophage-poor heart tissue showed scant FeCo/GC uptake, with the few spots of uptake colocalizing with macrophages (arrows).
In an experimental model of vascular inflammation, we have shown that a FeCo-based, graphite-coated nanoparticle can accumulate in vivo in vascular macrophages and can be imaged by fluorescence and MRI. To the best of our knowledge, this study is the first to show the use of FeCo or graphite-coated nanoparticles for in vivo macrophage imaging. We have previously reported that FeCo/GC exhibited higher T1 and T2 relaxivities than commercially available iron-oxide- and gadolinium-based contrast agents, with cell hyperthermia capabilities, and without evidence of in vitro or in vivo toxicity , . Furthermore, we have shown that FeCo/GC has a long circulation time and can allow very high-resolution MR angiography (down to 100 µm) . By demonstrating in vivo vascular macrophage uptake and imaging, we show that the potent MRI characteristics and potential therapeutic capabilities of FeCo/GC can be applied more broadly to atherosclerosis diagnosis and therapy – from high-resolution angiography to detection of vascular inflammation to macrophage thermal ablation.
Vascular inflammation has been studied by a variety of imaging modalities, including optical, nuclear, x-ray computed tomography, and MRI –. Prior optical studies have used bioluminescence, magneto-optical particles, or enzymatically activated near-infrared agents , , , , . MRI studies have primarily used ultra-small superparamagnetic iron-oxide agents for detecting macrophage infiltration in vascular lesions in both experimental and clinical studies –,  Gadolinium-based micelles and lipoproteins have also been used for macrophage MRI , . One study used a combined carbon nanotube/iron-oxide complex for macrophage cell imaging in vitro .
In addition to the advantageous MRI properties of FeCo/GC discussed above, FeCo/GC can be conjugated with targeting ligands or therapeutic drugs. We have also shown that the graphite shell provides high optical absorbance for photothermal therapy , while the FeCo component has the potential for magnetic hyperthermia . Thus, FeCo/GC nanoparticles have a wide range of imaging, targeting, and therapeutic capabilities and warrant further study.
While the carotid ligation model is advantageous in providing a discrete, macrophage-rich vascular lesion, it cannot replicate the complex, chronic plaques that develop in humans. Fluorescence imaging required in situ carotid exposure due to limitations in fluorescence tissue penetration. Fully noninvasive fluorescence imaging may be enabled with alternative techniques, such as fluorescence molecular tomography , . The MRI approach is likely made more challenging by using a carotid ligation model, as the ligation decreases both lumen size and flow. Aortic imaging in a transgenic hyperlipidemic mouse model is an alternative . Finally, while preliminary studies have shown no acute or chronic toxicity of FeCo/GC , more extensive, large-animal toxicity studies are needed prior to clinical translation.
In conclusion, the present study provides evidence that FeCo/GC nanoparticles are promising multi-modality contrast agents for vascular macrophage imaging. Further studies of this multi-functional nanomaterial may enable improved imaging, and therapy, of vascular inflammation in patients.
Materials and Methods
This study was carried out in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. The protocol was approved by the Administrative Panel on Laboratory Animal Care at Stanford University (Assurance # A3213-01). All procedures were performed under isoflurane anesthesia, and all efforts were made to minimize suffering.
A macrophage-rich murine carotid ligation model was used , . Eight-week-old male FVB mice (n = 17) were fed high fat diet containing 40% kcal fat, 1.25% (by weight) cholesterol and 0.5% (by weight) sodium cholate (D12109, Research Diets, Inc. New Brunswick, NJ, USA) . After 1 month on the diet, diabetes was induced by 5 daily intraperitoneal injections of streptozotocin (STZ, 40 mg/kg, Sigma-Aldrich, Saint Louis, MO, USA) dissolved in a citrate buffer (pH 4.5, Sigma-Aldrich, USA) . At day 5 of the STZ injections, serum glucose was measured from tail vein blood using a glucometer. If the glucose level was below 200 mg/dL, animals were injected with STZ for 3 additional days. Two weeks after the initiation of STZ injection, the left common carotid artery was ligated below the bifurcation with the use of 5-0 silk ligature (Ethicon) under 2% inhaled isoflurane . Sham operation was performed by passing the suture under the left carotid artery without constricting the artery. The wound was closed by suture and the animals were allowed to recover on a warming blanket.
The 7 nm FeCo/GC were synthesized as previously described , , then sonicated with 1 mg/mL phospholipid-polyethylene glycol (PL-PEG) in water for one hour. To obtain singly suspended FeCo/GC, the solution was centrifuged for 6 hours at 24,000× g. Excess PL-PEG was removed by filtration and UV-vis was used to determine nanocrystal and metal concentration.
For fluorescence imaging experiments the PL-PEG used was DSPE-PEG5000-NH2 (NOF corp.). For fluorescent dye attachment, Cy5.5-NHS ester was mixed with FeCo/GCPL-PEG-NH2 in phosphate buffered saline. Dye that was not attached to the nanocrystal was removed by filtration. Samples prepared for in vivo MRI imaging at 3 T were functionalized using DSPE-mPEG5000 (1,2-distearoyl-sn-glycero-3-phosphoethanolamine–N-[methoxy(polyethylene glycol)5000], Laysan Bio).
In vivo uptake and fluorescence imaging
To verify in vivo uptake of Fe/Co-GC in the carotid macrophages, Cy5.5 was conjugated to FeCo/GC, allowing fluorescence imaging and microscopy. FeCo/GC-Cy5.5 (8 nmol of Cy5.5/mouse; 32.14 µg Fe/mouse) was injected intravenously via tail vein into mice two weeks after carotid ligation (n = 6) or sham operation (n = 2). These mice were imaged at 48 hours using the Maestro™ in-vivo imaging system (Cri, Woburn, MA). Under inhalational anesthesia (2% isoflurane), left and right carotid arteries were surgically exposed and in situ florescence imaging was performed. Then, the carotid arteries were carefully removed en bloc followed by ex vivo fluorescence imaging and immunohistochemistry (see below).
In vivo MRI
To study noninvasive imaging of FeCo/GC by MRI, ligated mice (n = 6) were injected with FeCo/GC (270 µg Fe/mouse) and imaged serially at 48 and 72 hours on a whole-body 3T MRI scanner (Signa HDx, GE Healthcare) with a 50mT/m, 150T/m/s gradient system and a custom 3 cm surface radiofrequency coil. Another group of mice (n = 3) were injected with an 8-fold lower dose of FeCo/GC (32 µg Fe/mouse) and imaged at 48 hours on a small-bore 7T system (30 cm bore magnet, Varian Inc. plus GE “Micro-Signa” environment), with a 9 cm gradient insert (770mT/m, and 2500T/m/s, Resonance Research, Inc.) and a custom 6-cm RF coil. To detect the T2* effects of FeCo/GC, bright-blood images were acquired using gradient echo sequences (3T: repetition time (TR) = 100 ms, echo time (TE) = 10 ms, matrix size = 256×256, slice thickness = 1.0 mm, field of view (FOV) = 3 cm, flip angle = 60°; 7T: same parameters except TR/TE = 50 ms/4.2 ms, slice thickness = 0.5 mm). The slice position was matched using the aortic arch as a reference point.
For in situ carotid fluorescence imaging, regions-of-interest (ROIs) were placed on the left and right carotid regions and trachea. Average signal intensity divided by exposure time for left and right carotids was calculated and normalized to the trachea signal. For ex vivo carotid imaging, ROIs were placed around the entire left or right carotid artery and total signal intensity divided by exposure time was calculated. For in vivo MRI, FeCo/GC accumulation was assessed by measuring the extent of T2*-induced reduction in carotid lumen size, which was calculated as follows: % reduction of carotid lumen area = (1-[post-contrast carotid lumen area]/[pre-contrast carotid lumen area]) x 100% .
After euthanasia, carotid arteries were cut into two 3 mm sections. These sections, as well as liver and heart, were embedded immediately in optimum cutting temperature (OCT) compound (Sakura Finetek USA, Inc., Torrance, CA) and flash frozen in liquid nitrogen. Frozen sections (5 µm) were fixed in acetone for 10 minutes at 4°C . After sections were washed in PBS, they were incubated with anti-mouse Mac-3 antibody (BD Biosciences, San Jose, CA) or anti-mouse alpha smooth muscle actin antibody (Abcam Inc., Cambridge, MA) overnight at 4°C. Sections were then incubated with biotinylated secondary antibodies at room temperature for 30 minutes. Antigen-antibody conjugates were detected with avidin-biotin-horseradish peroxidase complex (Vector Laboratories, Burlingame, CA) according to the manufacturer's instructions. 3-amino-9-ethylcarbazole was used as chromogen. Sections were counterstained with hematoxylin.
Immunofluorescence double staining with confocal microscopy (Zeiss LSM 510, Carl Zeiss AG, Oberkochen, Germany) was performed to examine colocalization of FeCo/GC-Cy5.5 and macrophages. After incubation with anti-mouse Mac-3 antibody overnight at 4°C, sections were stained with Alexa Fluor 488-conjugated anti-rat IgG (Molecular Probes, Eugene, OR) at room temperature for 2 hours. Finally, sections were stained with DAPI (Sigma-Aldrich) to visualize cell nuclei.
All data are expressed as mean±SEM (standard error of the mean). Comparisons of fluorescence and MRI measures between left (ligated) and right (non-ligated) carotid arteries and between timepoints were analyzed by the Wilcoxon signed-rank test. Comparisons between ligated and sham left carotid arteries were analyzed by the Mann-Whitney U test. P<0.05 was considered statistically significant.
Conceived and designed the experiments: HK MT DGN HD MVM. Performed the experiments: HK SPS TK MT. Analyzed the data: HK TK MVM. Contributed reagents/materials/analysis tools: SPS JKB DGN HD. Wrote the paper: HK MVM.
- 1. Boyle JJ (2005) Macrophage activation in atherosclerosis: pathogenesis and pharmacology of plaque rupture. Curr Vasc Pharmacol 3: 63–68.
- 2. Libby P (2002) Inflammation in atherosclerosis. Nature 420: 868–874.
- 3. Hansson GK (2001) Immune mechanisms in atherosclerosis. Arterioscler Thromb Vasc Biol 21: 1876–1890.
- 4. Newby AC (2008) Metalloproteinase expression in monocytes and macrophages and its relationship to atherosclerotic plaque instability. Arterioscler Thromb Vasc Biol 28: 2108–2114.
- 5. Li W, Kornmark L, Jonasson L, Forssell C, Yuan XM (2009) Cathepsin L is significantly associated with apoptosis and plaque destabilization in human atherosclerosis. Atherosclerosis 202: 92–102.
- 6. Dahl TB, Yndestad A, Skjelland M, Øie E, Dahl A, et al. (2007) Increased expression of visfatin in macrophages of human unstable carotid and coronary atherosclerosis: possible role in inflammation and plaque destabilization. Circulation 115: 972–980.
- 7. Mauriello A, Sangiorgi G, Fratoni S, Palmieri G, Bonanno E, et al. (2005) Diffuse and active inflammation occurs in both vulnerable and stable plaques of the entire coronary tree: a histopathologic study of patients dying of acute myocardial infarction. J Am Coll Cardiol 45: 1585–1593.
- 8. Deguchi JO, Aikawa M, Tung CH, Aikawa E, Kim DE, et al. (2006) Inflammation in atherosclerosis: visualizing matrix metalloproteinase action in macrophages in vivo. Circulation 114: 55–62.
- 9. Amirbekian V, Lipinski MJ, Briley-Saebo KC, Amirbekian S, Aguinaldo JG, et al. (2007) Detecting and assessing macrophages in vivo to evaluate atherosclerosis noninvasively using molecular MRI. Proc Natl Acad Sci U S A 104: 961–966.
- 10. Hyafil F, Cornily JC, Feig JE, Gordon R, Vucic E, et al. (2007) Noninvasive detection of macrophages using a nanoparticulate contrast agent for computed tomography. Nat Med 13: 636–641.
- 11. Kolodgie FD, Petrov A, Virmani R, Narula N, Verjans JW, et al. (2003) Targeting of apoptotic macrophages and experimental atheroma with radiolabeled annexin V: a technique with potential for noninvasive imaging of vulnerable plaque. Circulation 108: 3134–3139.
- 12. Jaffer FA, Kim DE, Quinti L, Tung CH, Aikawa E, et al. (2007) Optical visualization of cathepsin K activity in atherosclerosis with a novel, protease-activatable fluorescence sensor. Circulation 115: 2292–2298.
- 13. Nahrendorf M, Zhang H, Hembrador S, Panizzi P, Sosnovik DE, et al. (2008) Nanoparticle PET-CT imaging of macrophages in inflammatory atherosclerosis. Circulation 117: 379–387.
- 14. Nahrendorf M, Waterman P, Thurber G, Groves K, Rajopadhye M, et al. (2009) Hybrid in vivo FMT-CT imaging of protease activity in atherosclerosis with customized nanosensors. Arterioscler Thromb Vasc Biol 29: 1444–1451.
- 15. Hyafil F, Laissy JP, Mazighi M, Tchétché D, Louedec L, et al. (2006) Ferumoxtran-10-enhanced MRI of the hypercholesterolemic rabbit aorta: relationship between signal loss and macrophage infiltration. Arterioscler Thromb Vasc Biol 26: 176–181.
- 16. Trivedi RA, Mallawarachi C, U-King-Im JM, Graves MJ, Horsley J, et al. (2006) Identifying inflamed carotid plaques using in vivo USPIO-enhanced MR imaging to label plaque macrophages. Arterioscler Thromb Vasc Biol 26: 1601–1606.
- 17. Howarth SP, Tang TY, Trivedi R, Weerakkody R, U-King-Im J, et al. (2009) Utility of USPIO-enhanced MR imaging to identify inflammation and the fibrous cap: a comparison of symptomatic and asymptomatic individuals. Eur J Radiol 70: 555–560.
- 18. Nahrendorf M, Jaffer FA, Kelly KA, Sosnovik DE, Aikawa E, et al. (2006) Noninvasive vascular cell adhesion molecule-1 imaging identifies inflammatory activation of cells in atherosclerosis. Circulation 114: 1504–1511.
- 19. Cormode DP, Briley-Saebo KC, Mulder WJ, Aguinaldo JG, Barazza A, et al. (2008) An ApoA-I mimetic peptide high-density-lipoprotein-based MRI contrast agent for atherosclerotic plaque composition detection. Small 4: 1437–1444.
- 20. Choi JH, Nguyen FT, Barone PW, Heller DA, Moll AE, et al. (2007) Multimodal biomedical imaging with asymmetric single-walled carbon nanotube/iron oxide nanoparticle complexes. Nano letter 7: 861–867.
- 21. Terashima M, Ehara S, Yang E, Kosuge H, Tsao PS, et al. (2010) In vivo bioluminescence imaging of inducible nitric oxide synthase gene expression in vascular inflammation. Mol Imaging Biol Epub Nov 6.
- 22. Terashima M, Uchida M, Kosuge H, Tsao PS, Young MJ, et al. (2011) Human ferritin cages for imaging vascular macrophages. Biomaterials 32: 1430–1437.
- 23. Seo WS, Lee JH, Sun X, Suzuki Y, Mann D, et al. (2006) FeCo/graphitic-shell nanocrystals as advanced magnetic-resonance-imaging and near-infrared agents. Nat Mater 5: 971–976.
- 24. Lee JH, Sherlock SP, Terashima M, Kosuge H, Suzuki Y, et al. (2009) High-contrast in vivo visualization of microvessels using novel FeCo/GC magnetic nanocrystals. Magn Reson Med 62: 1497–1509.
- 25. Fortin JP, Gazeau F, Wilhelm C (2008) Intracellular heating of living cells through Neel relaxation of magnetic nanoparticles. Eur Biophys J 37: 223–228.
- 26. Dong F, Li Q, Sreejayan N, Nunn JM, Ren J (2007) Metallothionein prevents high-fat diet induced cardiac contractile dysfunction: role of peroxisome proliferator activated receptor gamma coactivator 1alpha and mitochondrial biogenesis. Diabetes 56: 2201–2212.
- 27. Vallerskog T, Martens GW, Kornfeld H (2010) Diabetic mice display a delayed adaptive immune response to Mycobacterium tuberculosis. J Immunol 184: 6275–6282.
- 28. Harmon KJ, Couper LL, Lindner V (2000) Strain-dependent vascular remodeling phenotypes in inbred mice. Am J Pathol 156: 1741–1748.
- 29. Yu Z, Davis BB, Morisseau C, Hammock BD, Olson JL, et al. (2004) Vascular localization of soluble epoxide hydrolase in the human kidney. Am J Physiol Renal Physiol 286: F720–726.