| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
Basic Science Investigations |
1 Mallinckrodt Institute of Radiology, Washington University School of Medicine, St. Louis, Missouri
2 Department of Chemistry, Washington University, St. Louis, Missouri
3 Department of Radiology, University of Texas Southwestern Medical Center, Dallas, Texas
 |
ABSTRACT |
|---|
 TOP ABSTRACT INTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
Key Words: 64Cu • folate-nanoparticles • radiolabeling • folate receptor • enhanced permeability and retention effect
|
INTRODUCTION |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
Administered submicron particles are usually taken up by the macrophages of the reticuloendothelial system (RES), ending up in the liver, spleen, and lungs. However, a small size (<100 nm) and a hydrophilic surface can decrease nanoparticle opsonization and, consequently, slow down macrophages recognition (1,3,4).
To date, long-circulating nanoparticles have been evaluated mostly for delivery of antineoplastic agents such as doxorubicin, paclitaxel, 5-fluorouracil, irinotecan, and so forth, to solid tumors (4,5). Passively targeted delivery of drugs takes advantage of a defective vascular architecture caused by rapid tumor vascularization (angiogenesis), which is necessary for nutrient and oxygen supply and for waste disposal in fast-growing tumors (6). Blood vessels in solid tumors are highly permeable because of unusually large gaps (
300–800 nm) between adjacent endothelial cells caused by an abnormal arrangement of basement membrane and perivascular cells (7). However, a chaotic and disorganized branched vessel system and a high interstitial pressure result in pockets of nonaccessible cancer cells and make extravasation of blood-borne drugs difficult (6). Nonetheless, since tumors exhibit an impaired lymphatic system (8), macromolecules escaping RES sequestration may leak out of the permeable blood vessels and accumulate for a long time in perivascular tumor tissues (enhanced permeability and retention [EPR] effect) (4,5).
Alternative targeting approaches exploit the existence on target cells of molecular signatures for various pathologies. Thus, conjugation of ligands with high affinity for receptors, antigens, and so forth, overexpressed by tumor cells may allow early assessment and therapy of pathologies on a molecular level while decreasing cytotoxicity to normal tissues. To date, a variety of nanoparticles (nanospheres, nanocapsules, liposomes, dendrimers, and so forth) have been functionalized mainly with ligands and antibodies targeting endothelial receptors on tumor-proliferating microvasculature (2,9–13), the prostate-specific membrane antigen on prostate cancer cells (14,15), and the folate receptor (FR) (16–22).
The FR, or membrane-associated folate-binding protein, is 1 of the 2 existing cellular folate transport systems and binds physiologic folates with affinity in the nanomolar range (23). FR is an attractive molecular target for tumor targeting because it is overexpressed by several tumor cells (e.g., ovarian, colorectal, breast, nasopharyngeal carcinomas, and so forth), though it has only limited expression in most normal tissues (23,24). The feasibility of FR-mediated tumor delivery of drugs for therapy (22,25), of radionuclides for imaging (26), of vectors for gene delivery (21), and so forth, has been recently reviewed.
In this study, we evaluated in vivo and in vitro a new folate-conjugated polymeric nanoparticle for tumor targeting via both FR-mediated endocytosis and the EPR effect. Shell cross-linked nanoparticles (SCKs) are core-shell nanospheres inspired from biologic constructs and optimized for guest packaging (27). Stable SCKs are obtained by cross-linking the shell layer of micelles derived from the self-assembly of amphiphilic diblock copolymers in aqueous solution. Control over the synthesis of the diblock copolymers and the micellar formation conditions affords SCKs with well-defined size, surface charge, hydrophilicity, shape adaptability, and available functionality (27). To date, the SCK surface has been straightforwardly decorated with a variety of receptor ligands (13,17,28).
To evaluate the in vivo behavior of folate-SCKs, we have chosen 64Cu radiolabeling. 64Cu (half-life [t1/2] = 12.7 h) has been extensively studied for the production of radiopharmaceuticals for both PET and radiotherapy in the past 2 decades because of its radioactive decay with ß+ (17%) and ß– (40%) emission (29). At Washington University School of Medicine, no-carrier-added 64Cu is produced on a biomedical cyclotron with a high specific activity, suitable for receptor-targeting studies (30). For 64Cu-labeling purposes, the SCK-folate surface has been functionalized with 1,4,8,11-tetraazacyclotetradecane-N,N',N'',N'''-tetraacetic acid (TETA), a macrocyclic ligand that provides the copper complex kinetic and thermodynamic stabilty in vivo (29). Then, we evaluated the 64Cu-labeled SCK-folate nanoparticles in vivo in a tumor model overexpressing the FR (31). Biodistribution and autoradiography studies were performed to compare uptake and distribution of FR-targeted and nontargeted SCKs in KB tumor cell xenografts, thus evaluating the contribution of the EPR effect and FR-interaction to the tumor targeting. The present study is expected to have relevance in the understanding of active versus passive targeting of solid tumors via engineered nanoparticles. Furthermore, 64Cu-labeled nanoparticles may have the potential to deliver high concentration of radionuclide to solid tumors together with cytotoxic drugs, thereby enhancing the therapeutic efficacy and allowing imaging at the same time.
|
MATERIALS AND METHODS |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
/cm2) by passing through a Milli-Q water filtration system (Millipore Corp.). The buffer solution used for 64Cu-labeling reactions (0.1 mol/L ammonium acetate, pH 5.5) was further purified on Chelex 100 resin (Bio-Rad) before use. Centricon YM-100 tubes (100-kDa molecular weight cutoff) were purchased from Millipore Corp. 64Cu was prepared on the Washington University Medical School CS-15 cyclotron by the 64Ni(p,n)64Cu nuclear reaction at a specific activity of 47.4–474 GBq/µmol at the end of bombardment as previously described (30).
Synthesis of SCK and SCK-Folate
SCKs were prepared following a previously reported procedure (32). Briefly, the micelles were prepared in 2 steps from the diblock copolymer poly(acrylic acid-b-methyl acrylate) (PAA93-b-PMA164), as illustrated in Figure 1, followed by intramicellar crosslinking (20%) to produce shell cross-linked nanoparticles. A folate-PEG1,600-amine (PEG1,600 is a poly(ethylene glycol) spacer with a molecular weight of 1,600 Da) was also synthesized from folic acid and conjugated onto the shell surface of the SCKs by activating a portion of the available carboxylic acids with 1-(3'-dimethylaminopropyl)-3-ethylcarbodiimide (EDC) methiodide (13,17).
|
Synthesis of TETA-NH2
TETA-NH2 was synthesized in a straightforward way from TETA. Briefly, a mono tert-Boc–protected diamine (N-butoxycarbonyl-[2,2'-(ethylenedioxy)bis(ethylamine)]) was allowed to react with TETA in the presence of EDC for a period of 16 h. The protected intermediate was then isolated, the tert-Boc protecting group was cleaved with trifluoroacetic acid, and the TETA-NH2 product was then purified by repeated precipitation from methanol and acetone.
TETA Functionalization of SCK and SCK-Folate
The conjugation was done by a modified procedure developed for 1,4,7,10-tetraazacyclododecane-N,N',N'',N'''-tetraacetic acid (DOTA)-protein conjugation via the N-hydroxysuccinimide route (33). Briefly, the carboxylic groups on the SCK and SCK-folate shells were activated by adding EDC (2 equivalents with respect to the carboxylate groups) and N-hydroxysulfosuccinimide sodium salt (s-NHS) (4 equivalents with respect to the carboxylate groups). The activation reactions were performed in 10 mmol/L phosphate-buffered saline (PBS) solution (pH adjusted to 5.5) at 4°C for 2 h under gentle stirring. The s-NHS-SCKs were separated from excess EDC and s-NHS by Centricon YM-100 and the residues were extensively washed with PBS solution. The activated esters were reconstituted in 10 mmol/L PBS (pH 7.4) and then functionalized with TETA-NH2 (4 equivalents with respect to the carboxylate groups). The solution pH was adjusted to 8, and then the reaction mixtures were gently stirred at 4°C overnight. After TETA conjugation, the nanoparticle solutions were again concentrated by Centricon YM-100 and the residues were extensively washed with PBS to ensure complete separation from the unreacted TETA-NH2. Finally, the residues were reconstituted to 0.2–0.3 mg/mL solutions in 10 mmol/L PBS, pH 7.4, and stored at 4°C for further use.
Radiolabeling of TETA-SCK Conjugates with 64Cu
64Cu chloride (typically in 0.1 mol/L HCl) was converted to 64Cu acetate by adding 100 µL of 0.1 mol/L ammonium acetate buffer, pH 6.5. To 500 µL of the TETA-SCK solutions (in 10 mmol/L PBS, pH 7.4, containing 0.05% Tween 20), 50 µL of 64Cu acetate was added (185 MBq). The resulting solutions were incubated at 43°C for 2.5 h in a thermomixer (1,000 rpm). After incubation, the 64Cu/TETA-SCK solutions were added with 5 µL of 10 mmol/L diethylenetriaminepentaacetic acid (DTPA) and incubated for 10 min at room temperature. Radiochemical purity (RCP) of the 64Cu-labeled SCKs was determined by thin-layer chromatography (TLC) analysis after DTPA challenge, Centricon concentration, and washing. The solutions were spotted on silica gel TLC plates (Fisher Scientific), which were developed in methanol/10% ammonium acetate (v/v, 1:1) and analyzed by a Bioscan 200 imaging scanner (Bioscan Inc.). The 64Cu-labeled SCK remained at the origin, whereas the residual 64Cu-DTPA complex migrated with an Rf of 0.5 (labeling yield, 15%–20%, decay corrected; RCP, >95%). The products were then diluted with 0.05% Tween 20 solution in 10 mmol/L PBS, pH 7.4, to prepare appropriate doses for biodistribution and autoradiography studies.
Cell Culture
KB cells, a human nasopharyngeal epidermal carcinoma cell line overexpressing the FR (34), were obtained from American Type Culture Collection and cultured continuously as a monolayer at 37°C in a humified atmosphere containing 5% CO2 in folate-deficient modified Eagle’s medium (FDMEM) (a folate-free modified Eagle’s medium supplemented with 10% [v/v] heat-inactivated fetal bovine serum as only source of folate) containing 2 mmol/L L-glutamine.
Athymic Mouse Tumor Model
All animal studies were performed in compliance with guidelines set by the Washington University Animal Studies Committee. Three- to 4-wk-old female athymic nu/nu mice (Charles Rivers Laboratories) were used. After 1 or 2 wk on a folate-deficient rodent chow diet (ICN Biochemicals), mice were inoculated subcutaneously with 0.1 mL of KB cell suspension (1 x 106 cells per mouse) into the nape of the neck. SCK biodistribution studies were performed 1 wk after tumor cell implantation, when tumors reached 10- to 100-mg weight. For autoradiography studies, tumors were allowed to grow for 2 wk until they reached a 0.3- to 0.6-g weight. In both cases, mice were on a folate-deficient diet for 3 wk before radiotracer administration. Experiments with competitive block of the FR were performed by feeding the mice a normal rodent chow for 24 h and by administering them free folic acid (1 mg/100 µL 0.2 mol/L NaHCO3, by intraperitoneal injection) 24 h and 1 h before radiotracer administration.
In Vitro Cell Studies
KB cells in FDMEM were transferred to 33-mm culture dishes at 3 x 105 cells per dish 24 h before the assay. The cells were then rinsed with PBS (1 mL) and incubated for 4 h at 37°C or 4°C with 10 µg/mL of FTSC-SCK-folate diluted in culture medium. In free folate competition studies, 1 mmol/L folic acid was added to the incubation medium. After washing with PBS (3 x 1 mL) to remove free nanoparticles, cell-associated fluorescence was imaged by epifluorescence microscopy (Olympus IX-70 inverted microscope; Hitschfel Instruments Inc.). An argon laser for FTSC excitation at 488 nm was used for imaging.
Biodistribution Studies
64Cu-Labeled SCK and SCK-folate were diluted with 0.05% Tween 20 solution in 10 mmol/L PBS, pH 7.4. The KB tumor cell xenograft-bearing mice weighing 20–25 g (n = 4 per time point) were anesthetized with isoflurane and injected intravenously with 370–440 kBq of labeled nanoparticles (3–5 mg/kg mouse weight) in 100 µL via the tail vein. The mice were anesthetized before sacrifice (by cervical dislocation) at each time point. Organs of interest were removed and weighed, and sample radioactivity was measured. Standards were prepared and measured along with the samples to calculate the percentage injected dose per gram of tissue (%ID/g) and the percentage injected dose per organ (%ID/organ).
Autoradiography Studies
A 100-µL solution containing 1.85 MBq 64Cu-labeled SCK or SCK-folate (5 mg/kg mouse weight) was administered intravenously to KB tumor cell xenograft- bearing mice anesthetized with isoflurane (n = 2). The mice were then allowed access to food and water ad libitum. At 23 h after injection, the mice were anesthetized again and administered 18F-FDG (18.5 MBq in 100 µL) intravenously. At 24 h after injection, the mice were anesthetized and sacrificed by cervical dislocation. KB tumors were resected and sliced into 1-mm sections. Digital autoradiographs defining the intratumoral distribution of 18F radiotracer were collected (Canberra Packard Instant Imager; Canberra Industries Inc.) in a 2-min acquisition period shortly after the tumor was sectioned. After a 20-h delay, 64Cu images were collected with a 6-h acquisition period.
|
RESULTS |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
In Vitro Binding Studies
SCK-folate nanoparticles were labeled with FTSC and cell uptake was evaluated by epifluorescence microscopy after incubation of KB cells with 10 µg of nanoparticles at 37°C and 4°C. After 4 h of incubation at 37°C, folate-conjugated SCKs were found to bind KB cells and the fluorescence images suggest the presence of FTSC-SCK-folate–containing vesicles within the cytoplasm (Fig. 2A). After 4 h of incubation at 4°C, uptake of folate-conjugated SCKs on the KB cell surface was clearly visible, but no fluorescent vesicles were observed inside the cell (Fig. 2C). In both cases, FTSC-SCK-folate uptake could be blocked if free folate (1 mmol/L) was added to the binding medium during incubation (Figs. 2B and 2D).
|
Biodistribution Studies
Tables 1 and 2 present a summary of the biodistribution data for the 64Cu-TETA-SCK-folate and 64Cu-TETA-SCK conjugates in athymic nu/nu mice bearing small KB tumor cell xenografts (10–100 mg). Twenty mice were administered each radiolabeled nanoparticle. After intravenous injection, blood clearance was rapid and, after 10 min, blood uptake was constant (2–3 %ID/g) over the considered time points. For both nanoparticles, the highest %ID went to organs of the RES. Both SCKs were taken up rapidly by the liver (56.0 ± 7.1 %ID/g and 45.7 ± 3.5 %ID/g at 10 min after injection for SCK-folate and SCK, respectively) and were then slowly cleared through the intestine (21.5 ± 2.9 %ID/g and 26.9 ± 3.9 %ID/g liver uptake at 24 h after injection for SCK-folate and SCK, respectively). Similarly, spleen uptake was high shortly after nanoparticle administration (18.3 ± 6.3 %ID/g and 11.5 ± 2.5 %ID/g at 10 min after injection for SCK-folate and SCK, respectively) and then slowly decreased over time (4.7 ± 1.0 %ID/g and 4.5 ± 0.6 %ID/g at 24 h after injection for SCK-folate and SCK, respectively). 64Cu-Labeled SCKs were found to accumulate in lungs at 10 min after injection (39.7 ± 5.1 %ID/g and 32.5 ± 14.0 %ID/g for SCK-folate and SCK, respectively). However, unlike the liver and spleen, lung uptake of the SCK-folate was found to rapidly decrease within 1 h after injection (10.9 ± 3.8 %ID/g; P = 0.0001) and then remained constant throughout the rest of the experiment. Lung uptake of the SCK alone showed a similar profile, with a slightly slower clearance compared with the folate conjugate (15.0 ± 4.1 %ID/g and 12.7 ± 1.8 %ID/g at 1 and 24 h after injection, respectively). Among the non-RES organs, kidneys showed the same level of SCK-folate uptake over time (8–10 %ID/g), whereas heart uptake slightly increased from 2.3 ± 0.2 %ID/g at 10 min after injection to 4.3 ± 0.5 %ID/g at 24 h after injection. SCK uptake in these organs was slightly higher, yet with similar time distribution profiles.
|
|
|
5 mg/kg mouse weight) 24 h before sacrifice, to allow nanoparticle accumulation at the tumor site. Tissue distribution of nanoparticles was compared with 18F-FDG distribution by administering the mice with the 18F-labeled radiotracer (18.5 MBq) 1 h before animal sacrifice and tumor resection. Homogeneity of 18F-FDG and nanoparticle localization was evaluated on 1-mm tumor sections by acquiring images shortly after tumor resection and 20 h later, to allow for 18F decay. The collected images, depicted in Figure 4, showed nonhomogeneous distribution of both 64Cu-labeled nanoparticles and 18F-FDG within the tumor, with areas exhibiting no accumulation of either radiotracer. Furthermore, distribution of radiolabeled SCK was not in complete accordance with 18F-FDG distribution.
|
|
DISCUSSION |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
The FR is an attractive molecular target for radionuclide and drug delivery, since it is overexpressed by a panel of human cancers (23,24) and, in particular, by >90% of ovarian carcinomas, where receptor levels increase with tumor aggressiveness and grade (26).
A poly(ethylene glycol) (PEG) spacer with 34 repeat units (molecular weight, 1,600 Da) was introduced with the folic acid. Total numbers of ligands attached to the shell surface of these nanoparticles is another important parameter to achieve greater efficiency of interaction of nanoparticles with the cell-surface receptors. A theoretic calculation based on a procedure reported in the literature (35) showed that a total number of 20–70 folate-PEG1,600 is required to completely cover the surface of these 20 ± 3 nm nanoparticles. As a consequence, we functionalized 1% of the available COOH groups on the SCK surface, thus obtaining a nominal number of 90 folate-PEG1,600 per SCK, which is within the calculated range of the ligands to cover the whole surface.
Conjugation of FTSC on the nanoparticle surface allowed direct visualization of SCK-folate uptake in tumor cells in vitro by means of epifluorescence microscopy. The fluorescence images in Figure 2 show KB cells after 4 h of incubation in a solution containing FTSC-SCK-folate at 37°C (Fig. 2A) and at 4°C (Fig. 2C). In both cases, SCK-folate uptake on the cell surface is clearly visible. However, after incubation at 37°C, brightly fluorescent spots were visible inside the cells, suggesting the presence of SCK-folate in endocytotic vesicles. In contrast, after incubation at 4°C (temperature at which internalization is inhibited), no intracellular vesicles were visible and fluorescence was mainly limited to the cell surface. Furthermore, SCK-folate uptake at both 37°C and 4°C could be blocked if free folate (1 mmol/L) was added to the FTSC-SCK-folate solution during incubation (Figs. 2B and 2D). These findings confirm FR-mediated interaction between SCK-folate and FR-overexpressing tumor cells and suggest FR-mediated endocytosis in vitro, as previously observed for folate-conjugated liposomes (22) and other nanoparticles (20).
64Cu radiolabeling of SCK and SCK-folate was straightforward after TETA-NH2 conjugation. However, significant adsorption of 64Cu on the SCK surface was observed and a DTPA challenge was necessary to remove nonspecifically bound 64Cu activity from the nanoconjugates. As a consequence, moderate radiolabeling yields were achieved (15%–20%, decay corrected), but the high RCP (>95%, after DTPA challenge and Centricon purification) and the chemical stability (>60% intact 64Cu-TETA-SCK after 24 h of incubation at 37°C in PBS, as confirmed by radio-TLC analysis) were considered suitable for in vivo studies.
SCK-folate biodistribution and tumor-targeting capability were investigated in athymic nu/nu female mice bearing KB tumor cell xenografts. We chose 1-wk-old, small-size KB xenografts (10–100 mg) grown subcutaneously in the nape of the neck in mice to evaluate the possible use of nanoparticles to target early-stage solid tumors in vivo. Mice were kept on a folate-depleted diet before (3 wk) and during the experiments to achieve plasma folate levels in the physiologic range normally seen for humans (18). One day and again 1 h before each experiment, a group of mice was administered intraperitoneally excess folic acid to raise the plasma folate level and to evaluate the effects of competitive block of the FR on the SCK tumor uptake. As shown in Tables 1 and 2, administration of both folated and nonfolated 64Cu-labeled SCKs led to a rapid and extensive RES uptake. Folated SCKs showed higher accumulation in liver compared with nonfolated SCKs, reasonably because of higher opsonization and macrophage recognition after folate conjugation or to direct recognition by the liver FR (Kuppfer cell receptor–mediated endocytosis). Both SCK-folate and SCK exhibited also immediate lung uptake, probably due to sequestration of some aggregated nanoparticles by the lung capillary bed after intravenous injection. However, clearance of radiolabeled nanoparticles from lungs was fast and lung uptake values at 1 h after injection were in the range previously observed with other SCKs (data not shown).
Notwithstanding high RES uptake, the biodistribution data showed that SCKs had prolonged blood retention properties. Both folated and nonfolated SCKs were present in the blood at 24 h after injection (2.6 ± 0.6 %ID/g and 3.1 ± 0.3 %ID/g, respectively), with a slightly lower blood level of 64Cu-TETA-SCK-folate compared with the nonfolated conjugate due to higher liver uptake. As a result of the prolonged blood circulation, mice treated with radiolabeled SCKs showed in vivo tumor accumulation of radioactivity. However, the biodistribution data showed no evidence of the benefit of folate conjugation on in vivo accumulation of nanoparticles in FR-overexpressing tumors (Tables 1 and 2). Furthermore, the specific tumor uptake of both nanoparticles exhibited high variability within the groups of mice, resulting in high SDs.
Lack of selectivity of folate-conjugated nanoparticles and liposomes over nonfolated conjugates for FR-overexpressing solid tumors has been previously reported by other researchers (18,19,22,36,37). This is a result of passive extravasation from the permeable tumor blood vessels (EPR effect), which is the rate-determining step driving accumulation of long-circulating macromolecules in solid tumors. However, selective interaction of folated liposomes with FR-overexpressing cells in vivo has been demonstrated in ascitic tumor models (37,38).
Our biodistribution results confirm the nonspecific accumulation of nontargeted SCKs in solid tumors, but they also suggest FR-specific interaction of folated SCKs in small tumors. In fact, coadministration of excess folic acid led to competitive block of 64Cu-TETA-SCK-folate uptake in KB xenografts at 4 h after injection (Fig. 3A), whereas it had no noticeable effect on 64Cu-TETA-SCK uptake (Fig. 3B). Furthermore, SCK tumor uptake was seen to strongly depend on tumor weight: the smaller the tumor, the higher the specific SCK uptake. This is reasonably due to the presence of necrotic areas in big, fast-growing solid tumors, which hamper extravasation of blood-borne long-circulating molecules. This finding also explains the high variability in tumor uptake. In fact, tumor size varied considerably within each group and among different groups of mice used in the biodistribution study. However, effective uptake in small tumors is a key feature of potential systems for drug delivery, since it allows for the diagnosis and treatment of early-stage neoplasms.
SCK distribution in solid tumors was evaluated by means of dual-tracer autoradiography. In this series of experiments, we used mice bearing 2-wk-old subcutaneous KB tumor cell xenografts weighing 0.3–0.6 g. Mice were administered 64Cu-labeled SCKs and 18F-FDG separately, 24 and 1 h, respectively, before sacrifice. Digital autoradiography was then performed on 1-mm tumor slices shortly after sacrifice and 20 h later, to allow for complete 18F decay. Within tumor tissues, both 64Cu-labeled SCK-folate (Fig. 4A) and native SCK (Fig. 4B) exhibited a markedly heterogeneous distribution (which was confirmed in a second series of experiments, not reported here). In all tumor slices, sizeable zones appear that display no accumulation of either 18F-FDG or nanoparticles and that reasonably correspond to necrotic areas. However, despite the general concordance of regional 18F and 64Cu accumulation within the tumor, some areas exhibit accumulation of only one radiotracer, either 18F-FDG or 64Cu-labeled SCK. This is due to the different mechanisms driving the accumulation of the administered radiotracers. In fact, 18F-FDG is a small molecule that diffuses into tumor tissues and accumulates in areas of high metabolic activity (39), whereas macromolecules extravasate from hyperpermeable blood vessels and concentrate in vascularized tumor tissues regardless of tumor biochemistry.
Histopathologically, these KB cell tumor xenografts revealed apoptotic foci with macrophage infiltration and scattered necrotic areas (Fig. 5), consistent with autoradiographic findings.
|
|
CONCLUSION |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
Previously reported procedures for the synthesis of SCKs were followed with minor modifications, and a global solution-state functionalization strategy has been successfully developed for attaching optimum numbers of targeting and imaging agents onto the SCK nanoparticles. Epifluorescence microscopy confirmed the specific interaction of FTSC-conjugated SCK-folate with FR-overexpressing tumor cells in vitro. After TETA conjugation, we developed a simple method to radiolabel SCK and SCK-folate with 64Cu, which allowed us to perform in vivo biodistribution and autoradiography studies. Altogether, these studies confirmed that nanoparticle accumulation in solid tumors is achievable and that it is driven mainly by the EPR effect. In fact, both folated and nonfolated SCKs exhibited similar tumor uptake and distribution. However, FR-mediated uptake of SCKs in very small tumors was observed, suggesting the possible use of radiolabeled SCKs as drug delivery systems for imaging and treatment of early-stage tumors.
Although the focus of the current study has been on 64Cu labeling and FR targeting, the same strategy also applies to other imaging or therapeutic agents and molecular targets. SCKs are versatile and multivalent platforms, as their surface can be easily functionalized with a panel of different ligands, chelating systems, prodrugs, genes, and so forth, for a more broad-spectrum targeting approach.
|
ACKNOWLEDGMENTS |
|---|
|
FOOTNOTES |
|---|
For correspondence or reprints contact: Michael J. Welch, PhD, Mallinckrodt Institute of Radiology, Washington University School of Medicine, 510 S. Kingshighway Blvd., Campus Box 8225, St. Louis, MO 63110.
E-mail: welchm{at}mir.wustl.edu
|
REFERENCES |
|---|
|
TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONCONCLUSIONREFERENCES |
|---|
vß3-targeted nanoparticle and 1.5 tesla magnetic resonance imaging. Cancer Res. 2003;63:5838–5843.vß3 receptor-ligand interactions. Macromolecules. 2004;37:7109–7115.
This article has been cited by other articles:
|
|
 |
|
  R. Rossin, S. Muro, M. J. Welch, V. R. Muzykantov, and D. P. Schuster In Vivo Imaging of 64Cu-Labeled Polymer Nanoparticles Targeted to the Lung Endothelium J. Nucl. Med., January 1, 2008; 49(1): 103 - 111. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 R. L. Ehman, W. R. Hendee, M. J. Welch, N. R. Dunnick, L. B. Bresolin, R. L. Arenson, S. Baum, H. Hricak, and J. H. Thrall Blueprint for Imaging in Biomedical Research Radiology, July 1, 2007; 244(1): 12 - 27. [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| JOURNAL OF NUCLEAR MEDICINE TECHNOLOGY | THE JOURNAL OF NUCLEAR MEDICINE |
