Search tips
Search criteria 


Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Thromb Haemost. Author manuscript; available in PMC 2011 May 4.
Published in final edited form as:
PMCID: PMC3087830

Molecular imaging of macrophage protease activity in cardiovascular inflammation in vivo


Macrophages contribute pivotally to cardiovascular diseases (CVD), notably to atherosclerosis. Imaging of macrophages in vivo could furnish new tools to advance evaluation of disease and therapies. Proteolytic enzymes serve as key effectors of many macrophage contributions to CVD. Therefore, intravital imaging of protease activity could aid evaluation of the progress and outcome of atherosclerosis, aortic aneurysm formation, or rejection of cardiac allografts. Among the large families of proteases, matrix metalloproteinases (MMPs) and cysteinyl cathepsins have garnered the most interest because of their participation in extracellular matrix remodeling. These considerations have spurred the development of dedicated imaging agents for protease activity detection. Activatable fluorescent probes, radiolabeled inhibitors, and nanoparticles are currently under exploration for this purpose. While some agents and technologies may soon see clinical use, others will require further refinement. Imaging of macrophages and protease activity should provide an important adjunct to understanding pathophysiology in vivo, evaluating the effects of interventions, and ultimately aiding clinical care.


Innovations in imaging continue to revolutionize the practice of medicine by providing exquisite anatomical details that enhance diagnostic capabilities and enable monitoring of therapeutic interventions. In cardiovascular medicine, ultrasound, computed tomography (CT), nuclear, optical, and magnetic resonance imaging (MRI) provide high-resolution anatomic and functional images of the cardiovascular system, and x-ray fluoroscopy guides interventions to treat obstructive vascular disease and cardiac arrhythmias. Although many of these advanced imaging techniques provide excellent spatial resolution, in most cases they simply define anatomy or disease burden and provide physiologic information, rather than disclose information about the basic biological aspects of disease activity or therapies. Newer imaging strategies add to anatomic information by defining the cellular and molecular processes involved in cardiovascular disease (CVD), to improve understanding of the disease process, to obtain prognostic information, and to guide and follow cardiovascular therapies (1).

Inflammation plays a major role in CVD, and heightened inflammatory responses promote atherosclerosis, arterial thrombosis, vascular aneurysm formation, and rejection of transplanted hearts (24). Macrophages — mononuclear phagocytes in tissues derived from monocytes — operate as the major effectors of innate immunity in all of these CVD processes, often in response to signals from adaptive immune cells. Macrophage inflammatory functions that fight infection and promote tissue repair can turn against the host and promote disease progression. Thus, macrophages furnish an attractive target for the development of novel molecular cardiovascular imaging strategies, because these cells figure prominently in CVD, and hence macrophage-based imaging strategies might apply widely across the spectrum of cardiovascular disorders.

Molecular probes for macrophage imaging target several aspects of macrophage cell biology. Cellular probes specific for membrane markers on the cell surface can localize macrophages within tissues, and such surface proteins whose levels increase in stimulated cells can preferentially identify activated cells. Surface targets for macrophage imaging, although not specific for this cell type, include VCAM-1 (Vascular cell adhesion protein-1) (5), αvβ3 integrin (68), scavenger receptors (9, 10), ICAM-1 (Inter-Cellular Adhesion Molecule-1) (11), and CCR-2 9 (Chemokine (C-C motif) receptor 2) (12). In addition to localization by targeting surface proteins, internalization of probes through phagocytosis by macrophages can also detect such cells preferentially. Several nanoparticle-based, superparamagnetic probes show promise in this regard (13, 14). Stimulated phagocytes elaborate reactive oxygen species that could permit their detection. Macrophage proteases also hold promises as targets for cardiovascular imaging, because these enzymes (matrix metalloproteinases [MMPs] and cysteinyl cathepsins) function as important regulators of CVD processes and may comprise therapeutic targets for modulating disease activity.

Proteases belong to several families of enzymes that catalyze protein breakdown. These enzymes can exert endoproteolytic activity, exopeptidase activity, or both. Approximately 2% to 4% of a typical genome encodes proteolytic enzymes (15). The Degradome database, which does not incorporate protease pseudogenes or sequences derived from retroviruses, lists 569 human proteases and homologs classified into 68 families (16). Proteases fall into six groups, depending on their mechanism of action: serine, threonine, cysteine, aspartate, glutamic acid proteases, and MMPs (also known as matrixins). Mammals seem not to express glutamate proteases.

As uncontrolled proteinase action could prove catastrophic, several levels of regulation govern their expression and activity: regulation of gene expression; activation of precursor zymogens; blockade by endogenous inhibitors; targeting to specific compartments such as lysosomes, mitochondria, or membranes; and post-translational modifications. Proteinases control a variety of cellular and extracellular processes. Within cells, proteinases can regulate gene expression, cell differentiation and proliferation, or cell death, often through limited proteolysis. Outside of cells, proteinases participate in extracellular matrix protein turnover, in digestion of nutrients in the gut, and in host defenses and responses to tissue injury and healing (17, 18).

Molecular imaging in cardiovascular research mostly has focused on two families of proteases, produced abundantly by activated macrophages in inflamed tissues and implicated by considerable evidence in CVD: cysteinyl cathepsins and MMPs (19). This review will summarize the current state of the art of in vivo protease activity imaging in this context and highlight some recent alternatives for macrophage molecular imaging.

Imaging strategies and platforms for protease activity

Molecular imaging probes typically exhibit a targeting moiety that provides specificity linked to an imaging constituent (fluorophore, radionuclide, magnetic moiety, scatterer/absorber such as microbubbles, or photon generator such as luciferin) detectable by the imaging platform. In the case of extracellular proteinases, reporting on their activity conveniently does not require delivery of the probes to intracellular compartments.

Protease imaging has used two generic approaches: a) targeting labeled small molecules to specific protein pockets, typically the active site; and b) imaging substrates of proteases, which become activated and detectable upon cleavage. The first approach, commonly used with radionuclides, has wide application in clinical imaging with positron emission tomography (PET) or single-photon emission computed tomography (SPECT) platforms, especially because of their non-invasiveness, high versatility, and high sensitivity. Protease inhibitors (almost exclusively MMP inhibitors) have been labeled with 11C (20, 21) or with 18F (2224) for PET imaging in cancer. SPECT-labeled MMP inhibitors have undergone investigation in atherosclerosis (2528), vascular injury (29), and post-infarct remodeling (30). SPECT requires the use of isotopes like 99mTc, 111In, 123I, and 131I. To define the anatomical origin of the radioactive signals, both of these nuclear imaging platforms often combine with CT or MRI. The major limitations of PET and SPECT include low spatial resolution, exposure to radiation, a limited stoichiometry (one imaging probe per target enzyme), and the inability to differentiate protease-bound from unbound (circulating, sequestered, nonspecifically bound) imaging labels (Fig. 1).

Figure 1
Properties of imaging systems.

Like PET and SPECT, MRI instrumentation has wide availability in the clinical setting, and offers good spatial resolution and multicontrast capabilities. MRI used in coregistration with PET or fluorescent molecular tomography (FMT) provides fiducial anatomical references. MRI suffers, however, from lower sensitivity compared with radionuclide-based or optical approaches (Fig. 1). MRI technology relies on the interaction of water protons' magnetic moments in tissues with magnetic properties of the surrounding environment. By adding contrast agents that magnetically modify this environment, positive (T1- targeted) and negative (T2-targeted) enhancements can be generated and detected by MRI. The most commonly used untargeted contrasts agents are based on gadolinium, which shortens the spin-lattice relaxation time (T1) of nearby water protons. Studies have reported potential systemic toxicity of gadolinium, however, in patients with renal insufficiency (31). Superparamagnetic iron oxide nanoparticles, fluorine (19F)-carrying particles, manganese-based agents, and chemical exchange saturation transfer (CEST) agents are the current alternatives to contrast agents for increasing MRI sensitivity. For protease imaging in particular, studies have reported the development of specific inhibitors associated with magnetic agents (32, 33) and protease-sensitive magnetic nanoparticles (34, 35).

The use of enzyme-activatable selective fluorescent or magnetic substrates takes advantage of the enzyme’s catalytic activity. In this approach, each protease can convert many different imaging molecules. This property of labeled substrates provides the advantage of manifold amplification of the signal. One class of such “smart probes,” fluorescently-labeled substrates, produces intense fluorescence when cleaved due to separation from moieties that quench their fluorescence when in close proximity. Selectivity for certain enzymes derives from the sequence of the peptide-based substrate. In addition to avoiding radiation exposure, the near-infrared fluorescence (NIRF) imaging spectrum combines low autofluorescence and useful tissue penetration (millimeters to centimeters). Fluorescence signal can be acquired in surface-weighted mode by fluorescent reflectance imaging (FRI) or in tomographic mode (FMT), which employs mathematical algorithms that localize the origin of the fluorescence based on the NIRF diffusion in tissues (36). The tissue penetration of NIRF suffices for imaging of intact small animals such as mice, but would likely not permit external visualization of deep arteries (> 5–10 cm) in humans with today's technology. To overcome this limitation, a NIRF intravascular catheter approach in development could extend this technique to the imaging of proteinases related to inflammation in atherosclerotic human arteries (37).

Intravital confocal and multiphoton microscopy (IVM) also enables NIRF imaging. Despite limited application in humans due to its invasiveness, IVM provides high spatial resolution and sensitivity in experimental animals (Fig. 1). Multiphoton microscopy presents several advantages over confocal microscopy, including increased imaging depths and reduced out-of-focus photodamage. Multiphoton technology can also detect biological materials such as collagen, microtubules, and muscle myosin without any exogenous targeted agents by second harmonic generation (SHG) imaging.

Protease imaging can also be achieved with targeted microbubbles that permit imaging by contrast-enhanced ultrasound (CEU) (38, 39). Advantages of this approach include the widespread availability of suitable imaging platforms, the lack of ionizing radiation, and non-invasiveness. Disadvantages include lower inherent sensitivity, resolution, and penetration depth. Applied frequencies can currently achieve a resolution of <50 µm at reduced depth but this is not applicable when the structure of interest is located at deeper depths.

MMP imaging

In cardiovascular research and in protease imaging, the MMP collagenases and gelatinases have undergone the most extensive study because of their participation in degradation of macromolecules of the extracellular matrix — processes integrally involved in the remodeling of blood vessels and the myocardium (table I). In the inflamed atheroma and myocardium, proteinase activity increases compared to healthy tissues, in large part due to production by and release from macrophages (19, 40) (Fig. 5, upper panel).

Figure 5
Macrophage protease activity imaging in CVD.
Table I
Macrophage Protease Imaging Targets

In atherosclerosis, degradation of the collagenous extracellular matrix of the protective fibrous cap covering the lipid core of the plaque can lessen the lesion’s biomechanical strength. Rupture of the fibrous cap causes the majority of fatal acute myocardial infarcts by initiating thrombus formation (40). In the infarcting myocardium that is deprived of blood flow, ventricular remodeling may involve the extracellular matrix–degrading activities of MMP-2, MMP-9, and MMP-14 (41, 42). Elastolytic activity, potentially driven in part by MMP-9 and MMP-12, may promote aneurysm formation (43).

Proof-of-concept studies in mice have imaged gelatinase activity (MMP-2 and MMP-9) in vivo using an activatable NIRF substrate (44, 45). Confirmed by ex vivo FRI and in situ zymography, IVM and FMT imaging detected higher MMP and gelatinase activity in macrophage-rich atherosclerotic plaques and in infarct zones (Fig. 2). Recent studies on aneurysm formation also have succeeded in monitoring MMP activity by multimodality imaging, with FMT coregistered with CT to provide anatomical colocalization (46, 47); the intensity of MMP activity correlated with aneurysm development.

Figure 2
Fluorescence imaging of protease activity in mouse CVD.

Several publications have reported the generation of specific or broad-range MMP inhibitors (MMPI) labeled by radionuclides for PET/SPECT imaging. With a primary goal of screening of MMPI, broad spectrum hydroxamate pharmacophore MMPI have been coupled with 123I (48), 99mTc (30), and 18F (23, 24, 49) for SPECT or PET imaging (Fig. 3). Generation of MMP-2 and MMP-2/MMP-9 inhibitors, coupled with 18F (50) and 64Cu (51) or MMP-14 substrate radiolabeled with 99mTc, could permit more selective imaging of proteinases (52). Preliminary studies in atheromata, aneurysm, and wire-injured arteries correlated 99mTc- or 111In-MMPI signals with macrophages and MMP-2/MMP-9 activity in lesions by multimodal SPECT/CT imaging (25, 26, 5355).

Figure 3
MMPs imaging in vivo in atherosclerotic plaques by SPECT.

MRI-dedicated nanosensors for MMP-2/MMP-9 in development use nanoparticles loaded with the MR contrast agent gadolinium. Upon proteolysis, the nanoparticles exhibit highly cationic molecules that trigger attachment and intake into cells (35). Initial reports indicate a potential use for cancer targeting in vivo, but no study has yet assessed the utility of such agents in CVD. An MR probe for MMP-9 activity used charged nanoparticles with an iron oxide core coupled with methoxypoly(ethylene glycol) (MPEG) molecules, maintained in a stable state by a domain containing MMP-9 substrate (34). Upon MMP-9 cleavage, the remaining particles aggregated due to magnetic and electrostatic attraction. This study did not report In vivo MRI.

Cathepsin imaging

The cysteinyl proteinases included in the broad cathepsin (Cat) category also degrade matrix collagen and elastin (table I). Multiple reports implicate these enzymes in atherogenesis and in aneurysm formation (4, 56, 57). As in the case of MMPs, activatable NIRF probes can visualize cathepsin activity in vivo. An early study demonstrated the suitability of a Cat-B-dependent Cy5.5-labeled activatable NIRF probe for atherosclerosis imaging in vivo. In atherosclerotic mice after 24 weeks of consuming an atherogenic diet, FMT coregistered with MRI detected a strong signal in aortic plaques. In the same study, aortic aneurysms displayed high Cat-B activity assessed by ex vivo FRI. In contrast, arteries of healthy control mice yielded little signal. Histological analysis of the aorta after dissection confirmed a higher expression of Cat-B, colocalized with macrophages within lesions, as compared to healthy arterial tissue (58). A recent study demonstrated by ex vivo imaging that a similar probe could assess quantitatively the impact of anti-atherosclerotic treatments, such as statins, that reduced Cat-B activity in macrophage-rich plaques (59).

The potent elastolytic and collagenolytic protease Cat-K (57) that may contribute to plaque destabilization, aneurysm formation, and outward arterial remodeling during atherogenesis or following injury. In a study that used a NIRF imaging agent based on a Cat-K peptide substrate in vivo in mice, similar to the study described above involving Cat-B, optical imaging (IVM, ex vivo FRI) revealed more than twice as much signal in atherosclerotic mice and in human carotid endarterectomy specimens ex vivo, as compared with the control agent. The functional relevance of Cat-K was validated by fluorescent microscopy that colocalized Cat-K NIRF and Cat-K positive macrophages with fragmented elastin fibers within the media of underlying plaques (60).

Activity of the cysteinyl protease Cat-S associates with vascular calcification in mice with experimentally induced chronic renal disease (61). Injection of Cat-S activatable and osteogenesis-targeted imaging agents allowed the colocalization of Cat-S activity and calcification in aortas and aortic valves by IVM and ex vivo FRI. Cat-S–deficient mice exhibited less calcification and no Cat-S activity, validating the specificity of the probe and the involvement of the protease in this process.

In proof-of-concept studies, a broad cathepsin-activatable probe has sensed proteolytic potential in vivo in rabbit atherosclerotic lesions by an intravascular approach to overcome the limited-depth penetration of NIRF that precludes its clinical use for interrogation of deep arteries in humans (62). The same protease probe has visualized cathepsin activity experimentally in cardiac allografts undergoing rejection, and in myocardial infarcts. Seven days post-transplantation of histo-incompatible hearts without immunosuppression, myocardial graft rejection associated with accumulation of macrophages that produced active cathepsins, as visualized by FMT in vivo and FRI ex vivo by co-injecting the cathepsin probe and macrophage-targeted magneto-fluorescent nanoparticles. Macrophage recruitment was also imaged in vivo by MRI (13, 32, 33). In other experiments, co-injection of these two imaging agents four days after coronary ligation in mice demonstrated the active recruitment of macrophages and increased cathepsin activity in healing zones of the ischemic heart, as compared to healthy myocardium (14).

Cat-D is a lysosomal aspartyl protease that might play an important role in some cancers and in Alzheimer disease. Preliminary studies reported the development of Cat-D NIRF- and MRI-dedicated probes (63, 64).

Other targets for cardiovascular imaging of macrophage activity

In addition to MMP and cathepsin proteases, molecular imaging may prove useful for more extensively visualizing activity of macrophages via other enzymes or molecules that are especially relevant in CVD.

The enzyme myeloperoxidase (MPO) has received considerable interest as a biomarker for inflammation in atherosclerotic plaques and for future acute coronary events. Patients with stroke have elevated plasma MPO concentrations (65), and MPO levels seem to predict major cardiac events in patients presenting with acute chest pain (66) and in apparently healthy individuals (67). Although generally most abundant in granulocytes, within atheromata, MPO derives mainly from macrophages and macrophage-derived foam cells. MPO activity results in the generation of reactive oxygen species (ROS) — notably, hypochlorous acid (HOCl) — that may contribute to local alterations in arterial biology. In infarcting myocardium, MPO may also impede the healing remodeling process (68). A high level of MPO in plasma predicted an increase in five-year mortality for patients with acute MI (69). To assess MPO activity in vivo, a novel MPO sensor based on gadolinium permits detection of MPO by MRI (70). Studies in rabbits and mice reported high MPO activity, reflected by hyper-Zenhancement in diseased aortas and in infarct zones, when conventional gadolinium contrast would have subsided (Fig. 4)(68, 71, 72).

Figure 4
MPO activity following myocardial infarction (MI) by MRI.

Because macrophages play a key role in inflammatory CVD, they have received much attention as a target for molecular imaging. Iodinated, fluorescent, and/or magnetic nanoparticles based on an iron-oxide core phagocytosed by macrophages in plaques and in injured myocardium, can be imaged by optical or MRI or CT approaches (13, 14, 7375). 18F-fluorodeoxyglucose (18FDG) can track glucose uptake in macrophages. FDG signals colocalize with macrophage-rich inflamed sites in atheromata, as assessed in humans and in mice by SPECT/CT (7678). Uptake of 11C-choline or specific targeting imaging agents (99mTc-anti-RAGE antibody, 18F-galacto-RGD for αvβ3 integrin targeting, 99mTC-Annexin A5, 18F-radioligand for a mitochondrial benzodiazepine receptor) has undergone testing in experimental models of atherosclerosis (7, 7983).

Conclusion: Limits and future promises

Non-invasive molecular in vivo imaging, as an emerging technology, is a reality for several disease states but still requires refinement to progress into the clinical setting. In addition to the technological challenge for further increasing spatial resolution and sensitivity of the imaging hardware, a particular effort to improve or develop new imaging agents is crucial. For example, particle size and electrical charge are of great importance for the behavior of the agents in vivo, and therefore need to be carefully established. Moreover, future clinical applications for molecular imaging will require optimization of specificity, brightness (tissue penetration), and development of non-toxic agents.

Despite these current technological and cost-related limits, molecular imaging in general, and protease activity in particular, should contribute to biomedicine in the near future.

Detection of asymptomatic disease, and the prediction of severe complications, remains elusive to current diagnostic tools for many vascular disorders. Intravital imaging of protease activity promises to extend beyond anatomy and disclose biological aspects of the progress of atherosclerosis, myocardial infarct healing, heart transplant rejection, or aortic aneurysms. Moreover, novel therapeutic strategies in CVD should emerge from molecular imaging — including non-invasive imaging markers for prevention and personalized medicine, interventional imaging combined with treatment in the acute phase, and molecular assessment of therapeutic efficacy during treatment.

Preclinical studies in mice and rabbits have demonstrated how close we are to translating molecular imaging tools to the clinic. Imaging agents specifically targeting MMPs, cysteinyl cathepsins, or other enzymes implicated in CVD pathogenesis have demonstrated compatibility with established imaging platforms (PET, SPECT, MRI). The promising field of optical imaging will require special efforts in hardware to detect non-invasively small accumulations of active “smart probes” in inflamed or diseased tissues. Nonetheless, studies using MMPs and cathepsin-activatable probes have achieved proof of concept of the relevance and value of functional intravital imaging.

In addition to more reliable diagnosis and potential prediction of the outcome of a disease, molecular imaging for protease activity should also serve as a tremendous tool for development, evaluation, and dose ranging of novel therapeutics in vivo. Moreover, the coupling of imaging and therapeutic interventions with multifunctional nanoparticles opens the possibility of “theranostic” approaches. This concept involves targeting therapeutic drugs in particles carrying imaging moieties, for selective drug delivery to diseased tissues and simultaneous monitoring of not only targeting, but also possibly efficacy. In an illustration of such an approach, agents targeting scavenger receptor 1A on macrophages can detect MMP-9 activity (84). Multi-modality imaging — for example, tri-functional agents combining magnetic, optical, and radionuclide imaging functionality — promises to expand the gamut of molecular imaging (75, 8587). Such multimodal imaging agents must contain an adequate ratio of the various contrast agents for matching the relative sensitivity of the applied imaging modalities. This particular requirement may lead to the development of chemical constructs to create multiple binding sites of contrast agents, from which overall charge and size remain compatible with penetration into the targeted tissues (88).

Multimodal imaging strategies could also combine non-invasive and high-resolution technologies (e.g., confocal or multiphoton microscopy) to study protease activity in vivo, in interstitial as well as in intracellular milieu, to define their roles better and to characterize more precisely the behavior of imaging agents in the field of CVD. Current NIRF contrast agents, for example, may be applicable to combined FMT and (optical parametric oscillator-equipped) two-photon microscopy, where two-photon microscopy contributes both sub cellular resolution and imaging of intrinsic emission derived from extra cellular matrix components.

Protease imaging — and more broadly, molecular imaging — not only applies to CVD, but also to other diseases such as arthritis (89), asthma (90), and cancer (9193). Non-invasive intravital assessment of protease presence and activity will likely be feasible first by nuclear imaging in clinical trials, because of picomolar dosing and its widespread use in humans. The advantages of activatable probes over labeled inhibitors and the advent of multimodal imaging should increase efforts to introduce optical imaging into the clinic. The pace of progress in the development of novel molecular probes and imaging platforms during recent years highlights the promise of enabling advances in research and clinical applications through probing physiopathologic processes and assessment of specific molecular processes in intact subjects in vivo.


We thank our colleagues affiliated with the Donald W. Reynolds Clinical Cardiovascular Research Center at Harvard Medical School, who contributed to our efforts to develop molecular imaging of atherosclerosis and cardiovascular diseases. We also acknowledge the National Institutes of Health (R01-HL080472), the Translational Program of Excellence in Nanotechnology (TPEN) (U01 HL080731), and the American Heart Association for their support.


1. Ransohoff KJ, Wu JC. Advances in cardiovascular molecular imaging for tracking stem cell therapy. Thromb Haemost. 2010 Jul 5;104(1):13–22. [PMC free article] [PubMed]
2. Libby P. Inflammation in atherosclerosis. Nature. 2002 Dec 19–26;420(6917):868–874. [PubMed]
3. Mitchell RN, Libby P. Vascular remodeling in transplant vasculopathy. Circ Res. 2007 Apr 13;100(7):967–978. [PubMed]
4. Shimizu K, Mitchell RN, Libby P. Inflammation and cellular immune responses in abdominal aortic aneurysms. Arterioscler Thromb Vasc Biol. 2006 May;26(5):987–994. [PubMed]
5. Nahrendorf M, Jaffer FA, Kelly KA, et al. Noninvasive vascular cell adhesion molecule-1 imaging identifies inflammatory activation of cells in atherosclerosis. Circulation. 2006 Oct 3;114(14):1504–1511. [PubMed]
6. Chen W, Jarzyna PA, van Tilborg GA, et al. RGD peptide functionalized and reconstituted high-density lipoprotein nanoparticles as a versatile and multimodal tumor targeting molecular imaging probe. FASEB J. 2010 Jun;24(6):1689–1699. [PubMed]
7. Laitinen I, Saraste A, Weidl E, et al. Evaluation of alphavbeta3 integrin-targeted positron emission tomography tracer 18F-galacto-RGD for imaging of vascular inflammation in atherosclerotic mice. Circ Cardiovasc Imaging. 2009 Jul;2(4):331–338. [PubMed]
8. Wadas TJ, Deng H, Sprague JE, et al. Targeting the alphavbeta3 integrin for small-animal PET/CT of osteolytic bone metastases. J Nucl Med. 2009 Nov;50(11):1873–1880. [PMC free article] [PubMed]
9. Tawakol A, Castano AP, Gad F, et al. Intravascular detection of inflamed atherosclerotic plaques using a fluorescent photosensitizer targeted to the scavenger receptor. Photochem Photobiol Sci. 2008 Jan;7(1):33–39. [PMC free article] [PubMed]
10. Amirbekian V, Lipinski MJ, Briley-Saebo KC, et al. Detecting and assessing macrophages in vivo to evaluate atherosclerosis noninvasively using molecular MRI. Proc Natl Acad Sci U S A. 2007 Jan 16;104(3):961–966. [PubMed]
11. Choi KS, Kim SH, Cai QY, et al. Inflammation-specific T1 imaging using anti-intercellular adhesion molecule 1 antibody-conjugated gadolinium diethylenetriaminepentaacetic acid. Mol Imaging. 2007 Mar-Apr;6(2):75–84. [PubMed]
12. Hartung D, Petrov A, Haider N, et al. Radiolabeled Monocyte Chemotactic Protein 1 for the detection of inflammation in experimental atherosclerosis. J Nucl Med. 2007 Nov;48(11):1816–1821. [PubMed]
13. Christen T, Nahrendorf M, Wildgruber M, et al. Molecular imaging of innate immune cell function in transplant rejection. Circulation. 2009 Apr 14;119(14):1925–1932. [PMC free article] [PubMed]
14. Nahrendorf M, Sosnovik DE, Waterman P, et al. Dual channel optical tomographic imaging of leukocyte recruitment and protease activity in the healing myocardial infarct. Circ Res. 2007 Apr 27;100(8):1218–1225. [PubMed]
15. Puente XS, Sanchez LM, Gutierrez-Fernandez A, et al. A genomic view of the complexity of mammalian proteolytic systems. Biochem Soc Trans. 2005 Apr;33(Pt 2):331–334. [PubMed]
16. Quesada V, Ordonez GR, Sanchez LM, et al. The Degradome database: mammalian proteases and diseases of proteolysis. Nucleic Acids Res. 2009 Jan;37:D239–D243. (Database issue) [PMC free article] [PubMed]
17. Conus S, Simon HU. Cathepsins: key modulators of cell death and inflammatory responses. Biochem Pharmacol. 2008 Dec 1;76(11):1374–1382. [PubMed]
18. Fanjul-Fernandez M, Folgueras AR, Cabrera S, et al. Matrix metalloproteinases: evolution, gene regulation and functional analysis in mouse models. Biochim Biophys Acta. Jan;1803(1):3–19. [PubMed]
19. Libby P. Perplexity of plaque proteinases. Arterioscler Thromb Vasc Biol. 2006 Oct;26(10):2181–2182. [PubMed]
20. Zheng QH, Fei X, DeGrado TR, et al. Synthesis, biodistribution and micro-PET imaging of a potential cancer biomarker carbon-11 labeled MMP inhibitor (2R)-2-[[4-(6-fluorohex-1- ynyl)phenyl]sulfonylamino]-3-methylbutyric acid [11C]methyl ester. Nucl Med Biol. 2003 Oct;30(7):753–760. [PubMed]
21. Zheng QH, Fei X, Liu X, et al. Synthesis and preliminary biological evaluation of MMP inhibitor radiotracers [11C]methyl-halo-CGS 27023A analogs, new potential PET breast cancer imaging agents. Nucl Med Biol. 2002 Oct;29(7):761–770. [PubMed]
22. Breyholz HJ, Wagner S, Levkau B, et al. A 18F-radiolabeled analogue of CGS 27023A as a potential agent for assessment of matrix-metalloproteinase activity in vivo. Q J Nucl Med Mol Imaging. 2007 Mar;51(1):24–32. [PubMed]
23. Wagner S, Breyholz HJ, Holtke C, et al. A new 18F-labelled derivative of the MMP inhibitor CGS 27023A for PET: radiosynthesis and initial small-animal PET studies. Appl Radiat Isot. 2009 Apr;67(4):606–610. [PubMed]
24. Wagner S, Breyholz HJ, Law MP, et al. Novel fluorinated derivatives of the broad-spectrum MMP inhibitors N-hydroxy-2(R)-[[(4-methoxyphenyl)sulfonyl](benzyl)- and (3-picolyl)-amino]-3-methyl-butanamide as potential tools for the molecular imaging of activated MMPs with PET. J Med Chem. 2007 Nov 15;50(23):5752–5764. [PubMed]
25. Fujimoto S, Hartung D, Ohshima S, et al. Molecular imaging of matrix metalloproteinase in atherosclerotic lesions: resolution with dietary modification and statin therapy. J Am Coll Cardiol. 2008 Dec 2;52(23):1847–1857. [PubMed]
26. Haider N, Hartung D, Fujimoto S, et al. Dual molecular imaging for targeting metalloproteinase activity and apoptosis in atherosclerosis: molecular imaging facilitates understanding of pathogenesis. J Nucl Cardiol. 2009 Sep-Oct;16(5):753–762. [PMC free article] [PubMed]
27. Ohshima S, Petrov A, Fujimoto S, et al. Molecular imaging of matrix metalloproteinase expression in atherosclerotic plaques of mice deficient in apolipoprotein e or low-density-lipoprotein receptor. J Nucl Med. 2009 Apr;50(4):612–617. [PubMed]
28. Schafers M, Riemann B, Kopka K, et al. Scintigraphic imaging of matrix metalloproteinase activity in the arterial wall in vivo. Circulation. 2004 Jun 1;109(21):2554–2559. [PubMed]
29. Zhang J, Nie L, Razavian M, et al. Molecular imaging of activated matrix metalloproteinases in vascular remodeling. Circulation. 2008 Nov 4;118(19):1953–1960. [PMC free article] [PubMed]
30. Su H, Spinale FG, Dobrucki LW, et al. Noninvasive targeted imaging of matrix metalloproteinase activation in a murine model of postinfarction remodeling. Circulation. 2005 Nov 15;112(20):3157–3167. [PubMed]
31. Khurana A, Runge VM, Narayanan M, et al. Nephrogenic systemic fibrosis: a review of 6 cases temporally related to gadodiamide injection (omniscan) Invest Radiol. 2007 Feb;42(2):139–145. [PubMed]
32. Wu YL, Ye Q, Sato K, et al. Noninvasive evaluation of cardiac allograft rejection by cellular and functional cardiac magnetic resonance. JACC Cardiovasc Imaging. 2009 Jun;2(6):731–741. [PMC free article] [PubMed]
33. Ye Q, Wu YL, Foley LM, et al. Longitudinal tracking of recipient macrophages in a rat chronic cardiac allograft rejection model with noninvasive magnetic resonance imaging using micrometer-sized paramagnetic iron oxide particles. Circulation. 2008 Jul 8;118(2):149–156. [PMC free article] [PubMed]
34. Schellenberger E, Rudloff F, Warmuth C, et al. Protease-specific nanosensors for magnetic resonance imaging. Bioconjug Chem. 2008 Dec;19(12):2440–2445. [PubMed]
35. Olson ES, Jiang T, Aguilera TA, et al. Activatable cell penetrating peptides linked to nanoparticles as dual probes for in vivo fluorescence and MR imaging of proteases. Proc Natl Acad Sci U S A. 2010 Mar 2;107(9):4311–4316. [PubMed]
36. Ntziachristos V, Tung CH, Bremer C, et al. Fluorescence molecular tomography resolves protease activity in vivo. Nat Med. 2002 Jul;8(7):757–760. [PubMed]
37. Funovics MA, Weissleder R, Mahmood U. Catheter-based in vivo imaging of enzyme activity and gene expression: feasibility study in mice. Radiology. 2004 Jun;231(3):659–666. [PubMed]
38. Shalhoub J, Owen DR, Gauthier T, et al. The use of contrast enhanced ultrasound in carotid arterial disease. Eur J Vasc Endovasc Surg. Apr;39(4):381–387. [PubMed]
39. Lindner JR. Molecular imaging of cardiovascular disease with contrast-enhanced ultrasonography. Nat Rev Cardiol. 2009 Jul;6(7):475–481. [PubMed]
40. Libby P. The molecular mechanisms of the thrombotic complications of atherosclerosis. J Intern Med. 2008 May;263(5):517–527. [PMC free article] [PubMed]
41. Etoh T, Joffs C, Deschamps AM, et al. Myocardial and interstitial matrix metalloproteinase activity after acute myocardial infarction in pigs. Am J Physiol Heart Circ Physiol. 2001 Sep;281(3):H987–H994. [PubMed]
42. Kandalam V, Basu R, Abraham T, et al. TIMP2 deficiency accelerates adverse post-myocardial infarction remodeling because of enhanced MT1-MMP activity despite lack of MMP2 activation. Circ Res. 2010 Mar 5;106(4):796–808. [PubMed]
43. Hellenthal FA, Buurman WA, Wodzig WK, et al. Biomarkers of AAA progression. Part 1: extracellular matrix degeneration. Nat Rev Cardiol. 2009 Jul;6(7):464–474. [PubMed]
44. Chen J, Tung CH, Allport JR, et al. Near-infrared fluorescent imaging of matrix metalloproteinase activity after myocardial infarction. Circulation. 2005 Apr 12;111(14):1800–1805. [PMC free article] [PubMed]
45. Deguchi JO, Aikawa M, Tung CH, et al. Inflammation in atherosclerosis: visualizing matrix metalloproteinase action in macrophages in vivo. Circulation. 2006 Jul 4;114(1):55–62. [PubMed]
46. Kaijzel E, van Heijningen P, Wielopolski P, et al. Multimodality Imaging Reveals a Gradual Increase in Matrix Metalloproteinase Activity at Aneurysmal Lesions in Live Fibulin-4 Mice. Circ Cardiovasc Imaging. 2010 Jun 30; [PubMed]
47. Sheth RA, Maricevich M, Mahmood U. In vivo optical molecular imaging of matrix metalloproteinase activity in abdominal aortic aneurysms correlates with treatment effects on growth rate. Atherosclerosis. 2010 May 24; [PMC free article] [PubMed]
48. Breyholz HJ, Schafers M, Wagner S, et al. C-5-disubstituted barbiturates as potential molecular probes for noninvasive matrix metalloproteinase imaging. J Med Chem. 2005 May 5;48(9):3400–3409. [PubMed]
49. Breyholz HJ, Wagner S, Faust A, et al. Radiofluorinated pyrimidine-2,4,6-triones as molecular probes for noninvasive MMP-targeted imaging. ChemMedChem. 2010 May 3;5(5):777–789. [PubMed]
50. Furumoto S, Takashima K, Kubota K, et al. Tumor detection using 18F-labeled matrix metalloproteinase-2 inhibitor. Nucl Med Biol. 2003 Feb;30(2):119–125. [PubMed]
51. Sprague JE, Li WP, Liang K, et al. In vitro and in vivo investigation of matrix metalloproteinase expression in metastatic tumor models. Nucl Med Biol. 2006 Feb;33(2):227–237. [PubMed]
52. Watkins GA, Jones EF, Scott Shell M, et al. Development of an optimized activatable MMP-14 targeted SPECT imaging probe. Bioorg Med Chem. 2009 Jan 15;17(2):653–659. [PMC free article] [PubMed]
53. Ohshima S, Fujimoto S, Petrov A, et al. Effect of an antimicrobial agent on atherosclerotic plaques: assessment of metalloproteinase activity by molecular imaging. J Am Coll Cardiol. 2010 Mar 23;55(12):1240–1249. [PubMed]
54. Razavian M, Zhang J, Nie L, et al. Molecular imaging of matrix metalloproteinase activation to predict murine aneurysm expansion in vivo. J Nucl Med. 2010 Jul;51(7):1107–1115. [PMC free article] [PubMed]
55. Zhang Z, Mascheri N, Dharmakumar R, et al. Cellular magnetic resonance imaging: potential for use in assessing aspects of cardiovascular disease. Cytotherapy. 2008;10(6):575–586. [PMC free article] [PubMed]
56. Garcia-Touchard A, Henry TD, Sangiorgi G, et al. Extracellular proteases in atherosclerosis and restenosis. Arterioscler Thromb Vasc Biol. 2005 Jun;25(6):1119–1127. [PubMed]
57. Lutgens SP, Cleutjens KB, Daemen MJ, et al. Cathepsin cysteine proteases in cardiovascular disease. FASEB J. 2007 Oct;21(12):3029–3041. [PubMed]
58. Chen J, Tung CH, Mahmood U, et al. In vivo imaging of proteolytic activity in atherosclerosis. Circulation. 2002 Jun 11;105(23):2766–2771. [PubMed]
59. Kim DE, Kim JY, Schellingerhout D, et al. Molecular imaging of cathepsin B proteolytic enzyme activity reflects the inflammatory component of atherosclerotic pathology and can quantitatively demonstrate the antiatherosclerotic therapeutic effects of atorvastatin and glucosamine. Mol Imaging. 2009 Sep-Oct;8(5):291–301. [PubMed]
60. Jaffer FA, Kim DE, Quinti L, et al. Optical visualization of cathepsin K activity in atherosclerosis with a novel, protease-activatable fluorescence sensor. Circulation. 2007 May 1;115(17):2292–2298. [PubMed]
61. Aikawa E, Aikawa M, Libby P, et al. Arterial and aortic valve calcification abolished by elastolytic cathepsin S deficiency in chronic renal disease. Circulation. 2009 Apr 7;119(13):1785–1794. [PMC free article] [PubMed]
62. Jaffer FA, Vinegoni C, John MC, et al. Real-time catheter molecular sensing of inflammation in proteolytically active atherosclerosis. Circulation. 2008 Oct 28;118(18):1802–1809. [PMC free article] [PubMed]
63. Suchy M, Ta R, Li AX, et al. A paramagnetic chemical exchange-based MRI probe metabolized by cathepsin D: design, synthesis and cellular uptake studies. Org Biomol Chem. Jun 7;8(11):2560–2566. [PubMed]
64. Tung CH, Bredow S, Mahmood U, et al. Preparation of a cathepsin D sensitive near-infrared fluorescence probe for imaging. Bioconjug Chem. 1999 Sep-Oct;10(5):892–896. [PubMed]
65. Re G, Azzimondi G, Lanzarini C, et al. Plasma lipoperoxidative markers in ischaemic stroke suggest brain embolism. Eur J Emerg Med. 1997 Mar;4(1):5–9. [PubMed]
66. Brennan ML, Penn MS, Van Lente F, et al. Prognostic value of myeloperoxidase in patients with chest pain. N Engl J Med. 2003 Oct 23;349(17):1595–1604. [PubMed]
67. Meuwese MC, Stroes ES, Hazen SL, et al. Serum myeloperoxidase levels are associated with the future risk of coronary artery disease in apparently healthy individuals: the EPIC-Norfolk Prospective Population Study. J Am Coll Cardiol. 2007 Jul 10;50(2):159–165. [PubMed]
68. Nahrendorf M, Sosnovik D, Chen JW, et al. Activatable magnetic resonance imaging agent reports myeloperoxidase activity in healing infarcts and noninvasively detects the antiinflammatory effects of atorvastatin on ischemia-reperfusion injury. Circulation. 2008 Mar 4;117(9):1153–1160. [PMC free article] [PubMed]
69. Mocatta TJ, Pilbrow AP, Cameron VA, et al. Plasma concentrations of myeloperoxidase predict mortality after myocardial infarction. J Am Coll Cardiol. 2007 May 22;49(20):1993–2000. [PubMed]
70. Querol M, Chen JW, Weissleder R, et al. DTPA-bisamide-based MR sensor agents for peroxidase imaging. Org Lett. 2005 Apr 28;7(9):1719–1722. [PubMed]
71. Ronald JA, Chen JW, Chen Y, et al. Enzyme-sensitive magnetic resonance imaging targeting myeloperoxidase identifies active inflammation in experimental rabbit atherosclerotic plaques. Circulation. 2009 Aug 18;120(7):592–599. [PMC free article] [PubMed]
72. Ronald JA, Chen Y, Belisle AJ, et al. Comparison of gadofluorine-M and Gd-DTPA for noninvasive staging of atherosclerotic plaque stability using MRI. Circ Cardiovasc Imaging. 2009 May;2(3):226–234. [PMC free article] [PubMed]
73. Hyafil F, Cornily JC, Feig JE, et al. Noninvasive detection of macrophages using a nanoparticulate contrast agent for computed tomography. Nat Med. 2007 May;13(5):636–641. [PubMed]
74. Nahrendorf M, Waterman P, Thurber G, et al. Hybrid in vivo FMT-CT imaging of protease activity in atherosclerosis with customized nanosensors. Arterioscler Thromb Vasc Biol. 2009 Oct;29(10):1444–1451. [PMC free article] [PubMed]
75. Nahrendorf M, Zhang H, Hembrador S, et al. Nanoparticle PET-CT imaging of macrophages in inflammatory atherosclerosis. Circulation. 2008 Jan 22;117(3):379–387. [PMC free article] [PubMed]
76. Graebe M, Pedersen SF, Borgwardt L, et al. Molecular pathology in vulnerable carotid plaques: correlation with [18]-fluorodeoxyglucose positron emission tomography (FDG-PET) Eur J Vasc Endovasc Surg. 2009 Jun;37(6):714–721. [PubMed]
77. Reeps C, Essler M, Pelisek J, et al. Increased 18F-fluorodeoxyglucose uptake in abdominal aortic aneurysms in positron emission/computed tomography is associated with inflammation, aortic wall instability, and acute symptoms. J Vasc Surg. 2008 Aug;48(2):417–423. discussion 24. [PubMed]
78. Wu YW, Kao HL, Chen MF, et al. Characterization of plaques using 18F-FDG PET/CT in patients with carotid atherosclerosis and correlation with matrix metalloproteinase-1. J Nucl Med. 2007 Feb;48(2):227–233. [PubMed]
79. Fujimura Y, Hwang PM, Trout Iii H, et al. Increased peripheral benzodiazepine receptors in arterial plaque of patients with atherosclerosis: an autoradiographic study with [(3)H]PK 11195. Atherosclerosis. 2008 Nov;201(1):108–111. [PubMed]
80. Ishino S, Kuge Y, Takai N, et al. 99mTc-Annexin A5 for noninvasive characterization of atherosclerotic lesions: imaging and histological studies in myocardial infarction-prone Watanabe heritable hyperlipidemic rabbits. Eur J Nucl Med Mol Imaging. 2007 Jun;34(6):889–899. [PubMed]
81. Laitinen IE, Luoto P, Nagren K, et al. Uptake of 11C-choline in mouse atherosclerotic plaques. J Nucl Med. 2010 May;51(5):798–802. [PubMed]
82. Tekabe Y, Li Q, Rosario R, et al. Development of receptor for advanced glycation end products-directed imaging of atherosclerotic plaque in a murine model of spontaneous atherosclerosis. Circ Cardiovasc Imaging. 2008 Nov;1(3):212–219. [PubMed]
83. Pugliese F, Gaemperli O, Kinderlerer AR, et al. Imaging of vascular inflammation with [11C]-PK11195 and positron emission tomography/computed tomography angiography. J Am Coll Cardiol. 2010 Aug 17;56(8):653–661. [PubMed]
84. Suzuki H, Sato M, Umezawa Y. Accurate targeting of activated macrophages based on synergistic activation of functional molecules uptake by scavenger receptor and matrix metalloproteinase. ACS Chem Biol. 2008 Aug 15;3(8):471–479. [PubMed]
85. Jaffer FA, Libby P, Weissleder R. Optical and multimodality molecular imaging: insights into atherosclerosis. Arterioscler Thromb Vasc Biol. 2009 Jul;29(7):1017–1024. [PMC free article] [PubMed]
86. Silvera SS, Aidi HE, Rudd JH, et al. Multimodality imaging of atherosclerotic plaque activity and composition using FDG-PET/CT and MRI in carotid and femoral arteries. Atherosclerosis. 2009 Nov;207(1):139–143. [PMC free article] [PubMed]
87. Sinusas AJ, Bengel F, Nahrendorf M, et al. Multimodality cardiovascular molecular imaging, part I. Circ Cardiovasc Imaging. 2008 Nov;1(3):244–256. [PubMed]
88. Nahrendorf M, Keliher E, Panizzi P, et al. 18F-4V for PET-CT imaging of VCAM-1 expression in atherosclerosis. JACC Cardiovasc Imaging. 2009 Oct;2(10):1213–1222. [PMC free article] [PubMed]
89. Wunder A, Tung CH, Muller-Ladner U, et al. In vivo imaging of protease activity in arthritis: a novel approach for monitoring treatment response. Arthritis Rheum. 2004 Aug;50(8):2459–2465. [PubMed]
90. Cortez-Retamozo V, Swirski FK, Waterman P, et al. Real-time assessment of inflammation and treatment response in a mouse model of allergic airway inflammation. J Clin Invest. 2008 Dec;118(12):4058–4066. [PubMed]
91. Yang Y, Hong H, Zhang Y, et al. Molecular Imaging of Proteases in Cancer. Cancer Growth Metastasis. 2009 Aug 17;2:13–27. [PMC free article] [PubMed]
92. Weissleder R. Molecular imaging in cancer. Science. 2006 May 26;312(5777):1168–1171. [PubMed]
93. Weissleder R, Pittet MJ. Imaging in the era of molecular oncology. Nature. 2008 Apr 3;452(7187):580–589. [PMC free article] [PubMed]