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Published online before print April 14, 2006
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,1
* Divisions of Hematology and Oncology and
Pulmonary Medicine and
Laboratory Animal Research Core (LARC) Facility, Mayo Clinic Arizona, Scottsdale;
Department of Biological Sciences, Louisiana State University, Baton Rouge; and
¶ Department of Microbiology and Tropical Medicine, George Washington University, Washington, DC
1Correspondence: Division of Pulmonary Medicine, Department of Biochemistry and Molecular Biology, S. C. Johnson Medical Research Building, Mayo Clinic Arizona, 13400 East Shea Blvd., Scottsdale, AZ 85259. E-mail: jjlee{at}mayo.edu
ABSTRACT
Tumor-associated eosinophilia has been observed in numerous human cancers and several tumor models in animals; however, the details surrounding this eosinophilia remain largely undefined and anecdotal. We used a B16-F10 melanoma cell injection model to demonstrate that eosinophil infiltration of tumors occurred from the earliest palpable stages with significant accumulations only in the necrotic and capsule regions. Furthermore, the presence of diffuse extracellular matrix staining for eosinophil major basic protein was restricted to the necrotic areas of tumors, indicating that eosinophil degranulation was limited to this region. Antibody-mediated depletion of CD4+ T cells and adoptive transfer of eosinophils suggested, respectively, that the accumulation of eosinophils is not associated with T helper cell type 2-dependent immune responses and that recruitment is a dynamic, ongoing process, occurring throughout tumor growth. Ex vivo migration studies have identified what appears to be a novel chemotactic factor(s) released by stressed/dying melanoma cells, suggesting that the accumulation of eosinophils in tumors occurs, in part, through a unique mechanism dependent on a signal(s) released from areas of necrosis. Collectively, these studies demonstrate that the infiltration of tumors by eosinophils is an early and persistent response that is spatial-restricted. It is more important that these data also show that the mechanism(s) that elicit this host response occur, independent of immune surveillance, suggesting that eosinophils are part of an early inflammatory reaction at the site of tumorigenesis.
Key Words: tumor immunology • cancer • mice • B16 melanoma cells
INTRODUCTION
Galen [1 ] first noted the association between cancer and inflammation in his writings Opera Omnia almost 2000 years ago. During the succeeding millennia, the collective understanding of cancer-induced inflammatory responses evolved into a hypothesis first presented by Willis [2 ] that the human body recognizes and mounts a defensive response against tumors. A generation later, F. M. Burnet [3 ] characterized these responses, coining the term "immune surveillance". Since then, numerous studies have expanded the details of individual immune responses to tumors, including the recruitment of a variety of infiltrating lymphoid and myeloid cells. Moreover, many individual leukocyte subtypes have been investigated, and in many cases, the data suggest that they potentially participate in promoting or retarding tumor progression (reviewed in refs. [4 5 6 7 8 9 10 ]).
Despite an ever-increasing understanding of anti-tumor immune responses, several logistical problems have faced investigators studying the roles of leukocytes, preventing a comprehensive understanding of the relevant immune responses and the development of immune-based strategies to combat malignancies. For example, many tumors evade immune surveillance or elicit only nominal immune responses [11 12 13 ]. Cancers also often suppress immune responses, quenching otherwise effective defense mechanisms [14 15 16 ]. In addition, leukocyte infiltrates often vary with tumor type and size, suggesting that immune responses are neither consistent nor static events [6 , 17 ]. Investigations assessing these issues have led to the proposal that in addition to immune surveillance, host recognition of tumors also includes inflammatory responses [18 ]. Thus, in addition to specific immune-mediated responses, tumor sites are often centers of inflammatory reactions, leading to the recruitment of proinflammatory leukocytes [5 , 6 , 9 , 19 , 20 ].
Eosinophils have been recognized in cellular infiltrates of tumors, even in early histological studies of human cancers [21 22 23 24 25 ]. Clinical observations have shown that the appearance of eosinophils in solid tumors is common and occurs in several tumor types, particularly those of epithelial origin (e.g., colon and breast tumors; reviewed in refs. [21 , 26 ]). In some studies, this infiltrate was suggested as a positive, prognostic indicator of patient survival [27 28 29 30 31 ]; however, the design of these studies casts doubts on this claim (e.g., the lack of statistical power), preventing a definitive link between tumor growth and the presence of eosinophils. Despite the prevailing belief that eosinophils participate in anti-tumor mechanisms, the role of these leukocytes in host defenses against tumors is at best equivocal. Tumor growth clearly occurs despite the presence of eosinophils, including tumors in animal model systems, in which the malignant cells express eosinophil-agonist factors (see, for example, ref. [32 ]). The limited number of animal tumor models examined also fuels much of the controversy associated with eosinophils and tumor responses. For example, nearly all of the mouse studies examining eosinophils and eosinophil effector functions during tumorigenesis have used transfected cell lines modified to provoke defined immune responses in the recipient mice. In earlier studies, interleukin (IL)-4 was expressed [33 ], and in a more recent attempt [34 ], melanoma cells were genetically modified to express a specific antigen (ovalbumin) to elicit T helper cell type 2 (Th2) inflammatory responses in tumor-bearing mice sensitized to this antigen. The contrived character of these transfected cell models limits their translation to human disease, as it is unclear from any of these studies whether tumors are capable of recruiting eosinophils without the additional immune modulation of the tumor cells or the recipient mice. Moreover, the kinetic and spatial details of this tumor-associated eosinophilia in these models were often ignored, as eosinophil-specific antibodies for histological detection were unavailable.
The current study defines the parameters surrounding the recruitment and accumulation of eosinophils in the classical, well-defined B16 melanoma cell-derived tumor model. These studies used unmanipulated melanoma cells and wild-type mice, demonstrating that eosinophil recruitment to tumors was an early host inflammatory response that occurred, independent of Th2 immune responses. It is interesting that eosinophil accumulation occurred even in established tumors, and although the cause of this tumor-associated eosinophilia remains unresolved, evidence is presented, suggesting that the necrotic regions of tumors release a factor(s) that mediates eosinophil chemotaxis. Thus, the data presented demonstrate that eosinophil recruitment is spatially restricted to specific regions within tumors, occurs independent of immune surveillance mechanisms, and is likely an inflammatory response at the site of tumorigenesis, promoting an early and persistent host recognition of solid tumors.
MATERIALS AND METHODS
Animals
Recipient mice in melanoma cell injection studies (i.e., C57BL/6J) were purchased from The Jackson Laboratory (Bar Harbor, ME). All procedures were conducted on female mice, 8–16 weeks of age, maintained in ventilated microisolator cages, housed within a specific, pathogen-free animal facility, surveyed by a mixed-bed sentinel mouse program. Protocols and studies involving animals were conducted in accordance with National Institutes of Health (NIH; Bethesda, MD) and Mayo Clinic Foundation (Rochester, MN) institutional guidelines.
Generation of solid tumors
B16-F10 melanoma cells (American Type Culture Collection, Manassas, VA) were cultured in Dulbecco’s modified Eagle’s medium, supplemented with 10% heat-inactivated fetal calf serum (FCS) and 1% penicillin/streptomycin, all purchased from Invitrogen (Carlsbad CA). Melanoma cells (5x105) were injected subcutaneously (s.c.) above the right shoulder area of syngeneic C57BL/6J female mice. The site of injection was monitored daily, and the resulting solid tumors were allowed to grow until they were palpable (Day 10) or until the tumor weights averaged 
1 g (Day 16).
Histology and immunohistochemical detection of eosinophils
Mice were killed and tumors harvested for histological analysis, fixing the tissue overnight at 4°C in 10% formalin prior to embedding in paraffin. Serial 4 µm sections throughout the harvested tumors were stained with hematoxylin and eosin (H&E) or assessed for the presence of eosinophils by immunohistochemistry using a rabbit polyclonal anti-mouse eosinophil major basic protein (MBP) antiserum [35
]. Sections stained with biotin-conjugated rabbit immunoglobulin G (IgG; Sigma-Aldrich, St. Louis, MO) were included as an isotype control as described earlier [35
]. Immunohistochemical staining was performed with the VIP-Peroxidase detection kit (Vector Laboratories, Inc., Burlingame, CA) using a modified version of the protocol supplied by the manufacturer. Briefly, all slide manipulations were done at room temperature. Deparaffinized slides were hydrated in 1x phosphate-buffered saline (PBS) prior to the quenching of endogenous peroxidase activity in the tissue sections through a 20-min incubation in 0.6% H2O2/80% CH3OH. Quenched slides were washed in 1x PBS, digested with pepsin (10 min), washed again with 1x PBS, and finally, blocked with 1.5% normal goat serum (30 min). The rabbit polyclonal anti-mouse MBP antisera was used as a 1:1000 dilution in 1.5% normal goat serum and incubated with blocked slides for 60 min. Following three, 5-min rinses with 1x PBS/0.4% Tween-20, the slides were incubated with a biotinylated goat anti-rabbit secondary antibody, and MBP-specific antibody binding was visualized as a purple precipitate using the detection protocol outlined in the manufacturer’s instructions. The MBP-stained sections were counterstained with 0.1% methyl green in preparation for photomicroscopy, using an Axiotoplan microscope (Carl Zeiss, Obrkochen, Germany). The density of MBP-positive cells (i.e., eosinophils) within different regions of the tumors was quantified (cells/mm2) using the image analysis software program ImagePro Plus (Media Cybernetics, Silver Spring, MD).
Eosinophil-adoptive transfer and confocal microscopy
Adoptive transfers were performed using blood eosinophils isolated from IL-5 transgenic mice (NJ.1638 mice [36
]), back-crossed onto C57BL/6J (n>20 generations). Briefly, heparinized blood collected from several donors by cardiac puncture was layered onto a Percoll E gradient [60% Percoll E (
=1.084), 1x Hanks’ balanced saline solution (HBSS), 15 mM Hepes (pH 7.4)] and centrifuged (45 min, 3000 rotations per minute, 4°C). The eosinophil-enriched interface was recovered and washed twice in PBS containing 2% FCS. Eosinophils were isolated using a magnetic cell separation system (MACS, Miltenyi Biotec, Auburn, CA) through the elimination of contaminating B cells and T cells by positive selection with antibody-conjugated magnetic beads specific for CD45-R (B220) and CD90 (Thy 1.2), respectively. Cytospin preparations revealed that the recovered eosinophils were a nearly homogeneous population (>98.5% contaminating cells included 1% neutrophils and 0.5% monocytes), which displayed >99% viability via trypan blue exclusion.
The fluorescent marker, carboxylfluorescein diacetate (CFDA), was used to label purified peripheral blood mouse eosinophils as per the manufacturer’s instructions (Molecular Probes, Eugene, OR). CFDA-tagged eosinophils, 2 x 107 per animal, were transferred via the peritoneal cavity to tumor-bearing mice 24 h prior to tumor harvest (i.e., Day 15 of the melanoma cell-injection protocol). Frozen, serial, 4 µm sections were processed for confocal immunofluorescence microscopy using a coverplate system and a rat anti-mouse eosinophil-associated RNase (Ear) monoclonal antibody (mAb; Clone 32.2.3 [37 ]). Briefly, at room temperature, sections were washed twice with 1x PBS, blocked with 1% normal goat serum for 30 min, treated with 1% Chromotrope 2R (Aldrich, Milwaukee, WI) for 30 min, and then rinsed twice with 1x PBS/0.4% Tween-20. Individual slides were incubated with primary rat anti-mouse Ear antibody (diluted 1:1500) for 1 h at room temperature. Following incubation, the slides were washed two times with PBS, and an Alexa-568-conjugated goat anti-rat IgG secondary antibody (diluted 1:500; Molecular Probes) was added and incubated for 30 min at room temperature. Stained slides were washed twice with 1x PBS/0.4% Tween-20 prior to cover-slipping with Immu-mount (Themo Electron Corp., Pittsburgh, PA). CFDA and anti-Ear staining were evaluated using a Zeiss laser-scanning confocal microscope (LSM 510, Zeiss, Thornwood, NY). Negative control-stained sections revealed only nominal, nonspecific fluorescent staining of lung tissues.
Antibody-mediated depletion of CD4+ T cells
Anti-CD4 mAb (GK1.5) was used to deplete CD4+ cells using a modification of a protocol described previously [38
]. Briefly, GK1.5 was administered [intraperitoneally (i.p.)] to mice (0.5 mg/100 µl) 1 week prior to the s.c. injection of B16-F10 melanoma cells as well as on the day of melanoma cell injection. Tumor-bearing mice subsequently received additional administrations of GK1.5 antibody every 7 days until tumor harvest. Control groups of mice were administered nonspecific rat IgG. The ablation of CD4+ cells from mice was confirmed by flow cytometric analysis of splenocytes isolated from tumor-bearing mice. Spleen samples were disassociated into single cells by passage through a 40-µm mesh and repeated resuspension using a small pore pipette. Red blood cells were removed from the collected splenocytes with ammonium chloride lysis buffer, and the recovered white cells were washed in HBSS containing 2% FCS. Flurochrome-conjugated 
CD4 [fluorescein isothiocyanate (FITC)] and CD8 [phycoerythrin (PE)] mAb were used for staining (BD Biosciences, San Jose, CA). Analysis was performed on a FACScan flow cytometer (BD Biosciences) with CellQuest Pro software (BD Biosciences), gated to exclude fewer than 0.1% of the control cells in the relevant region for lymphocytes. Splenocytes derived from a tumor-bearing animal receiving nonspecific rat IgG were used to set the gates.
Ex vivo transwell assays of eosinophil chemotaxis assay
Transwell chemotaxis assays were performed using eosinophils isolated and purified (>98%) from the peripheral blood of IL-5 transgenic mice [36
] as described above. Eosinophil chemotaxis was determined via a transwell assay as described previously [39
]. The eosinophil chemotactic character of media from subconfluent cultures of mouse embryonic stem (ES) and B16-F10 melanoma cell cultures was tested as well as media from postconfluent B16-F10 melanoma cell cultures at defined times based on the percentage of dead cells present (i.e., cells grown beyond confluence in unchanged, nutrient-depleted media). Eotaxin-1 and -2 (PeproTech, Rocky Hill, NJ) were used at three concentration levels (3 nM, 10 nM, and 30 nM) as positive controls for migration, and culture media alone was used to determine the assay baseline (i.e., negative control). Data are expressed as a migration index, which is the number of cells that migrated in response to a chemotactic factor relative to the number of cells that migrated in response to media alone. Values presented are means ± SEM of duplicate determinations conducted on three separate occasions.
Statistical analysis
Unless otherwise noted, all data presented are mean values of the indicated groups (±SEM). Statistical analysis was performed on parametric data using Student’s t-test with differences between means considered significant when P < 0.05.
RESULTS
Subcutaneous injection of melanoma cells leads to solid tumors with characteristic regions of viable cells, areas of necrosis, and a surrounding acellular capsule/stromal layer
Subcutaneous injection of B16-F10 melanoma cells into syngeneic C57BL/6J mice (n=10 animals/group) resulted in well-developed, solid tumors as early as Day 10 postinjection with an average weight of 0.106 ± 0.03 g, which increased dramatically by Day 16, resulting in an average weight of 1.02 ± 0.17 g. Histological examinations of these tumors (Fig. 1
) revealed progressive growth with distinct regions of necrosis within viable regions. The small size of 10-day tumors was associated with a disproportionate amount of viable tissue relative to areas of necrosis, whereas the larger, 16-day-old tumors displayed extensive areas of necrosis. All tumors, irrespective of size, were surrounded by a largely fibrous acellular region (i.e., capsule) separating the tumor from surrounding host tissue.
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The onset and growth of cancers often appear to be a consequence of a tumor’s ability to avoid recognition by the host immune system and/or elicit immunosuppression (reviewed in refs. [46 47 48 ]). The lack of tumor-induced immune responses is clearly problematic for the host, limiting effective, immune-based defense mechanisms with which to eliminate and/or attenuate tumor growth. However, in contrast to the lack of immune-mediated responses, tumor-mediated changes at the site of growth may lead to the recruitment and accumulation of proinflammatory leukocytes [17 18 19 ]. Thus, although tumors are not necessarily immunogenic, the sites of growth often elicit an inflammatory response, which may represent an early host recognition mechanism of cancer.
The observations presented in this study suggest that the recruitment and accumulation of eosinophils to tumors are part of a site-specific, early host-recognition response. The eosinophil infiltration of B16-F10 melanoma cell-derived tumors occurred in all tumors examined without a concomitant induction of a marrow or peripheral blood eosinophilia beyond hemostatic baseline levels (i.e., without induced systemic-immune responses). This eosinophil infiltration also occurred following the s.c. injection of two other tumorigenic lines (Lewis Lung and CMT-93; data not shown), suggesting that the eosinophil infiltrate is a ubiquitous host response to solid tumor growth. In addition, this robust resident eosinophilia occurred even in the earliest palpable tumors. Significantly, the eosinophil tumor accumulation occurred without any additional immunomodulating events, as the injected melanoma cells were not manipulated to express a unique antigen (e.g., ovalbumin [34 ]) or an eosinophil-agonist cytokine/chemokine [25 , 33 , 49 ]. Moreover, the recipient wild-type mice were not allergen-sensitized/challenged to manipulate peripheral eosinophil numbers or their state of activation [34 ].
Several lines of evidence suggest that the B16-F10 melanoma cell-derived tumor itself and/or a host inflammatory response at the site of tumor growth are eliciting the accumulation of eosinophils. That is, the eosinophil infiltrate is not the result of acquired immunity or Th2-driven responses, which are part of larger host tumor surveillance mechanisms: The infiltration of tumors by eosinophils has been demonstrated in mice deficient of most acquired immune responses (e.g., in athymic nude mice [49 ]); B16 melanoma cells are syngeneic with the C57BL/6J recipient mice and do not elicit lymphocyte-mediated major histocompatibility complex-associated immune responses [50 ]; targeted depletion of all CD4+ cell types from recipient mice did not prevent the development of a tumor-associated eosinophilia; tumor growth did not induce an increase in eosinophilopoiesis, leading to an increase in circulating eosinophil numbers. In addition, the accumulation of eosinophils wasn’t simply an initial inflammatory response to tumor injection/establishment. Eosinophil-adoptive transfer showed that eosinophils accumulate even in established tumors, suggesting that their recruitment is an active, site-specific event, which occurs independently of T cell-mediated responses.
The observation that dead/dying, but not actively dividing, melanoma cells release one or more factors capable of mediating eosinophil chemotaxis suggests that the areas of necrosis and not the actively dividing, viable portions of the tumor may be the source of the factor(s) that result in the recruitment and accumulation of eosinophils. A cursory examination of several small molecule mediators released by stressed/dying cells failed to elicit eosinophil chemotaxis; however, other potential candidates remain to be examined that may contribute this chemotactic response, including various arachidonic acid metabolites suggested to have eosinophil-agonist activities (e.g., cysteinyl-leukotrienes [51 ], 5-oxo-eicosanoids [52 ], and lipid mediators such as platelet-activating factor [53 ]). Moreover, the observation that multiple cell types (transformed and nontransformed) also elicit this response suggests that this may be a more generalized mechanism mediated by a ubiquitous factor (e.g., high-mobility group box 1 [54 ]), which has a broader importance for eosinophil trafficking beyond recruitment to tumors. In addition, the ability of necrotic regions to induce eosinophil recruitment suggests that eosinophils are not trafficking to tumors as a secondary consequence of factors released by previously recruited leukocytes (i.e., inflammatory cells recruited prior to eosinophils).
Presumably, eosinophil recruitment occurs by migration from outside of the tumor through the capsule and viable regions, as these tumors display little evidence of vascularization, which would permit movement of eosinophils directly to the necrotic regions from circulation. In this model, the steady-state levels of accumulating eosinophils in each region of the tumor occurred as a consequence of a specific trafficking mechanism.
Necrotic regions
Eosinophils accumulate in the necrotic regions first and foremost, as this is the destination of the vectorial movement of these cells. Although the functionality of this accumulation remains unresolved, the ability of eosinophils to release copious amounts of vasoactive leukotrienes [55
] and potentially promote localized angiogenesis [56
, 57
] suggests that this eosinophilia may represent a physiologic response to localized hypoxia [58
]. This relationship between eosinophils and necrotic regions would also create a positive feedback loop, which may explain the increased eosinophil accumulation occurring as tumors become larger. That is, eosinophils recruited to necrotic regions of tumors may expand these areas of necrosis through destructive effector functions (e.g., release of toxic cationic proteins such as MBP) and increase the release of a chemotactic factor(s), which in turn, leads to the recruitment of yet more eosinophils.
Viable regions
The small, steady-state levels of resident eosinophils in the viable regions of the tumors may simply reflect the rapid transit of eosinophils, or alternatively, the absence of a significant resident population reflects the lack of stabilizing signals, prolonging eosinophil survival in these regions.
Capsule regions
The presence of a robust resident population of eosinophils in the capsule regions likely reflects the partial trapping of eosinophils, which are continually infiltrating from outside of the tumor as they attempt to move toward the necrotic regions [i.e., source of chemotactic factor(s)]. Alternatively, as the growing tumor crowds and physically perturbs the surrounding host tissue, the induced stress on these normal cells may lead to the release of remodeling signals, causing an initial influx of eosinophils to the tumor site prior to their subsequent response to the more localized chemotactic signals released by necrotic regions. This paradigm provides an explanation for our observation that eosinophil effector functions such as degranulation occur in the necrotic and not the capsule areas of tumors. The steady-state population of eosinophils in the capsule would not be expected to be necessarily activated or "functional", as these cells would be present only because of an inability to traverse this region efficiently or because of chemotactic signals released by the normal cells surrounding the growing tumor. In contrast, the necrotic regions of tumors are the sites toward which the eosinophils are moving because of a functional demand for eosinophil-mediated activities (i.e., the accumulation of eosinophils in this region is not a random event leading to the accumulation of "bystander" cells). Therefore, unlike other regions associated with the tumors, the necrotic areas promote eosinophil activation and the release of toxic cationic granule proteins (i.e., degranulation). Furthermore, eosinophil degranulation in the necrotic regions likely contributes to an overall loss of intact eosinophils from these regions, suggesting a mechanism leading to the lower steady-state levels observed in regions of necrosis relative to the capsule regions.
Regardless of the cause of accumulation or the mechanisms by which eosinophils traffic to tumors, a salient question remains: What are the consequences of this eosinophil infiltration? Specifically, are eosinophils destructive, cytotoxic effector cells limiting tumor growth as part of a host surveillance mechanism, or do the infiltrating eosinophils facilitate tumor growth by remodeling and immunoregulation of the tumor microenvironment? That is, do eosinophils promote the necrotic areas of tumors, which in turn, limits the rate of tumor growth, or are eosinophils recruited to tumors as a consequence of induced host inflammatory/tissue-remodeling responses? The absolute number of eosinophils in the necrotic areas of tumors, although significant, is relatively small (e.g., compared with macrophages [59 ]), which may limit the cytotoxic (i.e., destructive) effects potentially mediated by these granulocytes. In contrast, eosinophils are capable of elaborating numerous cytokines and growth factors that have agonist activities on remodeling events and immune responses (reviewed in ref. [60 ]) and have been linked to wound-healing [61 ], each consistent with hypotheses linking the induced recruitment to the necrotic areas of tumors to larger tissue-remodeling mechanisms.
The difficulties defining the role of these granulocytes in cancers occur because of the nominal character of the eosinophil infiltrate and the lack of studies of sufficient statistical power, demonstrating a link between eosinophils and modulations of tumor growth (see, for example, refs. [22 , 28 , 31 , 62 ]). Irrespective of these difficulties, tumors arise and grow despite the presence of an eosinophil infiltrate, and correlations with tumor growth have tended not to be linear (e.g., ref. [63 ] vs. ref. [34 ] vs. ref. [25 ]). Moreover, exceptions to the rule exist with apparent dissociations between the presence of eosinophils (and/or the lack thereof) and rates of tumor onset/growth (e.g., ref. [64 ]). In addition, all of the mouse studies attempting to causatively link the presence of eosinophils and modulations of tumor growth used genetically engineered the tumor cells [33 , 49 , 64 , 65 ] and/or immunized recipient mice to recognize the tumor cells [34 ], thus promoting the tumor as a target of Th2 inflammatory responses (i.e., an induced immune response vs. an elicited inflammatory response). Unfortunately, the narrow character of the models used as well as potential of pleiotropic effects mediated by the induction of contrived immune responses limit the usefulness of these approaches. However, the demonstration here that eosinophil infiltration is spatially restricted, even in the smallest tumors, and occurs independent of acquired immune responses suggests that this recruitment is part of an early host recognition of unique regional heterogeneities at the sites of tumorigenesis. It is more important that the understanding of the circumstances surrounding this tumor-associated eosinophil infiltrate provides a unique opportunity to define relevant effector functions that may represent novel, therapeutic options to modulation tumor onset/growth.
ACKNOWLEDGEMENTS
The work presented was supported by the Mayo Foundation and a grant from the National Cancer Institute to J. J. L. (CA112442-1S). Additional support was provided by NIH training grants to S. A. C. (AR08545 and AI07047-23) and S. I. O. (HL07897-07). We thank Dr. Pinku Mukherjee for her assistance with the ex vivo chemotaxis studies as well as the invaluable contributions of numerous individuals not listed as authors. We also thank the tireless efforts of the Mayo Clinic Arizona core facilities [Laboratory Animal Resources Core (LARC): Dr. Ron Marler; Histology: Lisa Barbarisi; Immunology: Tammy Brehm-Gibson; Medical Graphic Arts: Marv Ruona; Research Library Services: Joseph Esposito]. Mr. Tim Jensen and Dr. Helene Rosenberg provided insightful comments and critical review of early versions of this manuscript. In addition, we express our gratitude to the Lee Laboratories administrative staff [Linda Mardel, Margaret (Peg) McGarry, and Jennifer Ford], without whom we could not function as an integrated group.
FOOTNOTES
1 Correspondence: Division of Hematology and Oncology, Department of Biochemistry and Molecular Biology, S. C. Johnson Medical Research Building, Mayo Clinic Arizona, 13400 East Shea Blvd., Scottsdale, AZ 85259. E-mail: nlee{at}mayo.edu 
Received January 13, 2006; revised February 7, 2006; accepted February 28, 2006.
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