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Inflammation occurs routinely when managing gliomas and is not easily distinguishable from tumor re-growth with current magnetic resonance imaging (MRI) methods. The lack of non-invasive technologies that monitor inflammation prevents us to understand whether it is beneficial or detrimental for the patient, and current therapies do not take this host response in consideration. We aim to establish whether a gadolinium (Gd)-based agent targeting the inflammatory enzyme myeloperoxidase (MPO) can selectively detect intra- and peri-tumoral inflammation as well as glioma response to treatment by MRI.
We performed serial MPO-Gd-MRI before and after treating rodent gliomas with different doses of oncolytic virus (OV) and analyzed animal survival. The imaging results were compared to histo-pathological and molecular analyses of the tumors for macrophage/microglia infiltration, virus persistence and MPO levels.
Elevated MPO activity was observed by MRI inside the tumor and in the peritumoral cerebrum at day 1 post-OV, which corresponded with activation/infiltration of myeloid cells inhibiting OV intratumoral persistence. MPO activity decreased as the virus and the immune cells were cleared (days 1–7 post-OV), while tumor size increased. A ten-fold increase of viral dose temporally decreased tumor size, but augmented MPO activity, thus preventing extension of viral intratumoral persistence.
MPO-Gd-MRI can distinguish enhancement patterns that reflect treatment-induced spatio-temporal changes of intratumoral and intracerebral inflammation from those indicating tumor and peritumoral edema. This technology improves the post-treatment diagnosis of gliomas and will increase our understanding of the role of inflammation in cancer therapy.
Management of brain tumors induces inflammatory responses that interfere with tumor imaging and monitoring the treatment course. Inflammation may also influence the outcome of the therapy in two opposite ways. It can lead to tumor control, by killing cancer cells and establishing an anti-cancer immunity (1–8), or to tumor promotion, by participating in glioma reoccurrence and progression (9–17). It is thus important to establish a non-invasive imaging technique that monitors intracerebral inflammation and distinguishes it from tumor in order to understand the clinical and physiological consequences of this host response, and to efficiently diagnose the outcome of cancer treatments that enhance or inhibit local inflammation.
Oncolytic viruses (OV) present a great potential for the treatment of malignant gliomas, due to their capacity to replicate in situ and reach peripheral invasive cancer cells. However, OV are very immunogenic and, despite their replication capacity, are rapidly cleared from the tumor by inflammatory cells that engulf virus-infected cancer cells (18–23). Because OV-induced inflammation is rapid and precisely localized, it is an optimal model to establish techniques for in vivo imaging of intra-cerebral inflammation during glioma treatment.
Myeloperoxidase (MPO) is an inflammatory enzyme present in myeloid cells (neutrophils, microglia, and macrophages). It is secreted during inflammation by activated, pro-inflammatory subsets of these cells (24). MPO utilizes hydrogen peroxide to catalyze the formation of reactive oxygen species that: kill pathogens, covalently modify lipids, cause local damage, and further activate the inflammatory cascade (24, 25). Gd-bis-5-HT-DTPA (MPO-Gd) is a molecular magnetic resonance imaging (MRI) agent that reports MPO activity with high specificity and sensitivity (26–31). This agent has been validated in vivo to evaluate MPO activity and inflammation in atherosclerosis (32), experimental autoimmune encephalomyelitis (33), stroke (26), and myocardial ischemia (28). Imaging of MPO activity is possible because of a prolonged gadolinium (Gd) enhancement caused by MPO-mediated oxidation of the Gd-chelating agent which induces its polymerization and trapping in the tumor mesh (26, 27, 30, 34). Therefore, immediately after MPO-Gd administration the MRI highlights areas of vessel leakage in the tumor and allows measurement of tumor size, whereas prolonged enhancement observed 1–2 hours after injection of the agent reflects MPO activity.
We have investigated the possibility of using MPO-Gd-MRI to analyze intratumoral and intracerebral inflammation during glioma treatment with OV and tested whether such inflammation was associated with improved therapeutic response. To do this, we have examined the patterns of MPO-Gd-MRI contrast enhancement in two different rodent glioma models (the rat D74-HveC and the mouse CT-2A gliomas) treated with different doses of the oncolytic herpes simplex virus hrR3 (35), and compared the imaging results with the extent of intratumoral/intracerebral infiltration/activation of inflammatory cells, viral load, MPO levels, and animal survival.
Our results indicate that MPO-Gd MRI reports the in vivo spatiotemporal evolution of the OV-induced inflammatory response and provides a powerful tool to understand the role of inflammation during glioma OV-treatment.
D74/HveC rat glioma cells (36) were grown in Dulbecco’s modified Eagle medium (DMEM) supplemented with 10% fetal calf serum (FCS) and 7.5 µg/mL blasticidin S (Calbiochem®, EMD Biosciences Inc., La Jolla, CA, USA); CT-2A mouse glioma cells [provided by Dr. Thomas Seyfried, Boston College (37)] were grown in DMEM with 10% FCS.
Male Fischer 344 rats (Taconic Farms Inc., Germantown, NY, USA) and C57BL/6J mice (NCI, Frederick, MD) were kept according to the guidelines of the Subcommittee on Research Animal Care of MGH. Tumors were implanted using stereotaxy as described (36). Seven days after implantation, 105 or 106 plaque forming units (pfu) of hrR3 or equivalent volume of phosphate buffer (PBS) were injected in the tumor using the same procedure and stereotactic coordinates as for the cancer cells.
Total RNA from the anterior quarter of the tumor-bearing cerebrum was extracted with the RNeasy Lipid Tissue kit (Qiagen, Valencia, CA, USA), from animals treated with virus (106 or 105 pfu) or PBS (5 µl) for 1, 3, or 6 days. Three animals for each treatment-group/virus-dose/time-point were used. cDNA was synthesized using the Omniscript™ Reverse Transcriptase Kit (Qiagen, 205113) and random primers (Invitrogen, Carlsbad, CA). TaqMan PCR was performed with the ABI Prism® 7000 HT Sequence detection system and TaqMan PCR Master Mix (Applied Biosystems, Foster City, CA, USA). PCR reaction mix included a 25 µL aqueous solution containing each primer at 0.9 µM, the probe at 200 nM, and 2 µL of diluted cDNA. The PCR program included 1 cycle of 2 minutes at 50°C, 1 cycle of 10 minutes at 95°C, and 40 cycles comprising 15 seconds at 95°C followed by 1 minute at 60°C. 18S rRNA was used as internal control. Relative quantification of gene expression was calculated as 2ΔCt lacZ or MPO/2ΔCt r18S, ΔCt = difference between the numbers of cycles needed to reach saturation for the same gene in two different treatment groups. Primers: LacZ forward–tgttgccactcgctttaatgat, reverse–actcgccgcacatctgaact, probe-6FAM-cgctgtactggaggc-TAMRA; 18S rRNA forward-gggcccgaagcgtttact, reverse-ttccctagctgcggtatcca, probe-6FAM-caaagcaggcccgagccgc-TAMRA; MPO forward-tggctggagtgcgatcttc, reverse-cgtgcatctgccagtttgag, probe-6FAM-tgaggccgatactgtc-TAMRA.
Rodent brains from animals treated with 105 pfu of virus or 5 µl PBS for 1, 3 or 9 days (3 animals/treatment-group/time-point) were frozen in an isopentane dry-ice bath and sectioned through the entire tumor volume. Every fifth section was collected for analysis. Tissue slides were fixed in ice-cold acetone, and stained as follows. After blocking endogenous proteins and peroxidases with serum-free protein block (X0909) and peroxidase-blocking reagent (002428) (DAKO-Cytomation, Glostrup, Denmark), sections were incubated 1 hour at room temperature with the following primary antibodies (all antibodies from Serotec, Kidlington, Oxford, UK, except for MPO antibody from Neomarkers, Fremont, CA): mouse anti-rat CD68 (MCA 341R) and CD163 (MCA 342R), rat anti-mouse F4/80 (MCA497RT), and rabbit anti-human Myeloperoxidase (Ab-1). For bright-field staining the slides were then incubated with a horseradish peroxidase-conjugated (HRP) secondary antibody (ECL anti-mouse IgG, NA931V, Amersham Biosciences Ltd, Little Chalfont, Buckinghamshire, UK, and anti-rabbit IgG BA-1000, Vector Laboratories, Burlingame, CA), a Liquid DAB Substrate Chromogen System used for detection (K3465, DAKO-Cytomation), and hematoxylin for counterstaining. For fluorescent staining the slides were incubated with an anti-rat IgG-FITC secondary antibody (Jackson Immunology, West Grove, PA, cat# 115-095-166) and mounted with propidium-iodide Vectashield mounting medium H-1300 (Vector Laboratories, Burlingame, CA).
The paraffin embedded human brain sections were deparaffinized, rehydrated, and treated with 1% Sodium Dodecyl Sulphate before staining. The rabbit anti-human Myeloperoxidase (Ab-1) (Neomarkers), mouse anti-human CD68 and CD163 (AbD Serotec P34810 and Q86VB7) were used with the same secondary antibodies as above.
Intratumoral viral spread was analyzed by detecting β-galactosidase activity with X-gal (5-bromo-4-chloro-3-inodolyl-β-D-galactopyranoside, Sigma-Aldrich, St. Louis, MO).
The anterior quarter of the tumor-containing cerebrum treated with 105 pfu of virus or 5 µl of PBS for 1, 3 or 6 days (5 animals/group/time-point) was extracted, weighed, and homogenized in 50 mM potassium phosphate buffer at pH 6.0. After centrifugation, the pellet was re-suspended in cetyltrimethylammonium bromide buffer (Sigma-Aldrich), homogenized again, and sonicated. After three cycles of freeze-thaw-sonication, the cell lysates were centrifuged and the supernatants were collected. Protein concentration was measured with the BCA Protein Assay kit (23225, Pierce, Thermo Fischer Scientific, Rockford, IL). The protein extracts were then used to measure MPO activity by detecting Amplite ADHP (AAT Bioquest, Sunnyvale, CA) oxidation through spectrophotometry at 535 nm. The units of activity were computed according to the formula: activity (U/mL) = (ΔOD × Vt × 4)/(E × Δt × Vs) where ΔOD is the change in absorbance, Vt is the total volume, Vs is the sample volume, E is the extinction coefficient=3.9 × 104 M−1s−1, and Δt is the change in time. The resulting activity was normalized to 1 mg of protein or 1 mg of tissue to derive the specific activity. The specificity of the MPO activity was tested by adding 4-aminobenzyoic acid hydrazide to the protein lysates before the spectrophotometric reading (38).
Rats treated with 105 or 106 pfu of virus or 5 µl PBS for 1, 3 or 7 days (3 animals/treatment-group/viral-dose/time-point) were anesthetized with isoflurane (2.0 % at 2 L/min) and imaged using a 4.7-Tesla, 16-cm bore MRI system (Bruker Pharmascan, Billerica, MA). Rats were imaged one day before and 1, 3 and 7 days after injection of hrR3. MR images were acquired before and for 2 hours after the intravenous administration of MPO-Gd [synthesized as previously described (29) from DTPA-Gd (Magnevist, Berlex Laboratories), and injected at 0.3 mmol/kg mouse and 0.1 mmol/kg rat] using a T1-weighted rapid-acquisition with refocused echoes (RARE) sequence (repetition time [TR] = 800 ms, echo time [TE] = 13 ms, matrix [MTX] = 192 × 192, slice thickness = 1.0 mm, number of excitations [NEX] = 8, field of view [FOV] = 2.5 cm for mouse and 3.5 cm for rats). T2-weighted imaging was also performed (TR=4217 ms, TE=60 ms, MTX = 192 × 192, slice thickness = 0.8 mm, NEX = 8, FOV is the same as for T1-weighted sequences). Standard DTPA-Gd was used in control animals to verify that MPO-Gd enhancement was specific for MPO activity.
Regions of interest (ROI) including the tumor, contralateral brain tissue, and muscle were selected using the freeware OsiriX (www.oxirix-viewer.com). Contrast-to-noise ratios (CNRs) were computed for each ROI with the formula: CNR = (postcontrast ROIlesion −postcontrast ROImuscle)/SDnoise) − (precontrast ROIlesion − precontrast ROImuscle)/SDnoise), where ROIlesion is the ROI of the enhancing areas, and SDnoise is the standard deviation of noise measured from an ROI placed in an empty area of the image. CNRs were normalized by dividing each CNR by the highest CNR to enable comparison between different animals. Activation ratios (ARs) were computed by dividing the CNR of the late phase (75 minutes) over the CNR of the early phase (first post-contrast images, 5 minutes) to account for nonspecific enhancement from leakage. Tumor radius was computed by measuring the maximum transverse dimension.
Comparisons between multiple groups were performed with 2-sided ANOVA test followed by means comparisons with post hoc Tukey’s test using the software Prism (Graphpad Software Inc. La Jolla, CA). Comparison between two groups was performed using the student t-test. A p-value < 0.05 was considered to be statistically significant. All error bars indicate SEM.
We have previously established that treatment of a rat glioma with hrR3 induces intratumoral recruitment of mature peripheral macrophages (CD68+/CD163+) and activation of brain inflammatory cells (CD68+/CD163−) that accumulate around the tumor borders (19, 20). To use OV-treatment as a model for establishing in vivo imaging techniques of intracerebral/intratumoral inflammation, we analyzed the kinetics of CD68+ and CD163+ cells activation/recruitment during treatment of the D74-HveC rat glioma with hrR3 beginning one day post viral injection to a point when the animals appeared moribund (6 days from PBS injection in control animals, and 9 days from viral dosing in treated rats), which was considered as end of therapy. Because both these inflammatory cells subtypes engulfed hrR3-infected cancer cells (19, 20), we compared this kinetic profile with the kinetics of viral clearance.
The virus was gradually and completely cleared from the tumor between day 1 post viral dosing and the end of therapy (Figure 1). The intratumoral viral concentration matched with activation/infiltration of CD68+ and CD163+ cells which were prominent at day 1 post virus (compared to animals receiving PBS), decreased at day 3, and were similar to control in moribund animals.
Because brain inflammatory cells produce high levels of MPO (31, 39), we hypothesized that MPO-Gd-MRI could monitor OV-induced infiltration and activation of CD68+ and CD163+ cells. To test this hypothesis, we analyzed whether the kinetics of activation/infiltration of these inflammatory cells and viral clearance corresponded to changes in MPO mRNA levels and enzymatic activity (Figure 2). For this assay, rats with established D74-Hvec gliomas were treated with PBS (controls) or hrR3 and sacrificed at days 1, 3 and 6 after virus injection. We chose 6 days as the last time point because of the high mortality of the control rats. We found that more than 90% of viral LacZ mRNA is cleared from the tumor between days 1 and 3 and the remainder is cleared by day 6 (undetectable by RT-PCR, Figure 2A). Accordingly, we observed the highest levels of MPO mRNA and activity at day 1 post viral dosing and both significantly decreased by day 3 (Figure 2B–D). No MPO mRNA levels were detected by RT-PCR in control animals and at day 6 after virus injection, however, we could still observe some MPO activity in both these situations (Figure 2B,C). The decrease of MPO activity between days 3 and 6 was not very strong in OV-treated animals and demonstrated a high variability among animals, suggesting that intratumoral decrease of macrophages is ongoing but not yet fully established as observed when rats appear moribund (Figure 2C). Because it is impossible to precisely dissect the tumor tissue from adjacent cerebrum these assays do not distinguish between intratumoral and peritumoral MPO activity. However, IHC staining of rat brains harboring gliomas and treated with OV or PBS clearly shows the presence of MPO in both the intratumoral and peritumoral areas (Supplementary Figure S1), thus matching the distribution of CD68+ and CD163+ cells observed in Figure 1.
We have previously reported on the similarity of inflammatory cellular responses in mice and rats carrying human or syngeneic gliomas treated with different types of OV (19, 20, 22, 23). Accordingly, comparison of hrR3 spread in the CT-2A mouse glioma between 6 and 72 hours from OV injection showed that most of the intratumoral virus was cleared within 3 days of delivery, and this matched with infiltration of F4/80+ macrophages (Figure 3A), as well as increased MPO mRNA levels and enzymatic activity (Figure 3B). Moreover, the GBM from a patient treated with the oncolytic adenovirus ONYX-015 (40) also presented infiltration of CD68+ and CD163+ cells (20) expressing MPO (Supplementary Figure S2).
Altogether, these data indicate that the inflammatory response induced by OV is associated with MPO mRNA levels and enzymatic activity. This phenomenon is not species-specific and suggests the possibility to image inflammation in vivo with MPO-Gd-MRI.
We determined if MPO-Gd-MRI could detect the kinetics of CD68+ and CD163+ cells activation/infiltration observed by IHC and distinguish the areas of inflammation from the bulk tumor tissue. We imaged rats carrying D74-HveC tumors 1 day pre-viral dosing for tumor baseline signal, and 1, 3 and 7 days post-hrR3 (Figure 4). Each imaging session included analysis of tumor size (we measured the diameter of the region enhancing 5 minutes after injection of the MPO-Gd contrast agent), and quantification of the MPO activation ratio (determined by analyzing the persistence of the contrast 75 minutes after injection of MPO-Gd). We could not image the animals after day 7 post viral dosing because of a rapid health decline.
Before viral dosing (day 0) the MPO-Gd enhancement faded over time during the imaging session, indicating low MPO activity (Figure 4A). At days 1 and 3 post-virus, the MPO-Gd contrast decreased comparably slower inside the tumor center and increased in the parenchyma surrounding the tumor (Figure 4A). Calculation of the MPO activation ratio from MPO-Gd-MRI showed a 3-fold increase between days 0 and 1 and a trend of decrease from day 1 to 7 (Figure 4C), which matched with the MPO activity measured through the enzymatic assays (Figure 2C). At day 7 most of the enhancement in the center of the tumor faded 75 minutes after MPO-Gd injection (Figure 4A,C) and few CD163+ macrophages were detected by histopathology in these tumors (Supplementary Figure S3). However, there was persistence of MPO-Gd contrast at the periphery between the tumor and the brain parenchyma and histopathology revealed accumulation of CD68+ cells in the same regions (Supplementary Figure S3). MRI performed at day 1 after OV treatment using standard DTPA-Gd as contrast agent indicated rapid leakage of this agent from the tumor tissue and adjacent brain (Figure 4B,D). These results demonstrate that MPO-Gd contrast enhancement comes from MPO secreted by two distinct cell populations, inside and surrounding the treated tumor, reflecting a difference in the host response to OV therapy.
Comparison of images obtained through MPO-Gd MRI with those obtained using dextran-coated iron oxide particles (MION), which are incorporated by phagocytes and confer superparamagnetic properties to these cells (41), on animals treated with hrR3 for 3 days indicates that these two technologies for in vivo imaging of immune cells overlap only partially. MION imaging did not detect the peritumoral area of inflammation visible through MPO-Gd MRI, but had a broader distribution inside the tumor (Supplementary Figure S3).
Analysis of tumor size (Figure 4E) indicated tumor growth between days 0 and 1. This growth was slower between days 1 and 3 post-hrR3 injection, and became again pronounced between days 3 and 7. The retardation of tumor growth observed between days 1 and 3 is likely due to the oncolytic activity of the virus and was not observed in animals treated with PBS. Notably, the overall trend of tumor size change after virotherapy, as reported on the diameters measured by MRI at 5 minutes after delivery of the contrast agent, is opposite of the trend of in vivo MPO activity measured from delayed images (75 minutes post MPO-Gd, compare Figures 4C and 4E), underscoring that this technology can distinguish areas of inflammation from the tumor tissue.
We then imaged and measured hrR3-mediated induction of MPO activity with MPO-Gd MRI in mice carrying the CT-2A glioma (Figure 5). Also in this case, we detected a spatiotemporal change in the enhancement pattern between the early and delayed images, which differentiated tumor from inflammation. We found that increased in vivo MPO activity reported by molecular MRI following viral treatment matched with the infiltration of F4/80+ monocytic cells (Figure 3) and with increased MPO activity measured through enzymatic assays on excised tumors (Figure 3), suggesting that this technology is applicable to different species.
To further match the MPO-Gd contrast enhancement with changes in virus-induced inflammation, we compared rats treated with 2 different doses of hrR3 (105 and 106 pfu). Increasing viral load at the time of injection did not change the time frame with which the virus is completely cleared; i.e. at seven days no virus was detected through RT-PCR in either treatment group (data not shown). One day after virus injection there was 10-fold difference in LacZ between these two treatment groups that related to the difference of viral dose, but the MPO mRNA levels were similar (Figure 6A,B). At day 3, the difference in LacZ mRNA between these two treatment groups was only about 2-fold and the group receiving the higher viral dose had increased MPO mRNA (Figure 6A,B). This corresponded to increased MPO activity measured by MPO-Gd-MRI (Figure 6C) and smaller tumor size (Figure 6D).
We have shown that the myeloid cells activated in the brain and infiltrating the tumor upon OV treatment induce MPO, thus allowing MR-imaging of their inflammatory activity through a gadolinium-based molecular imaging agent (27, 29). Our data indicate that the kinetics of intracerebral/intratumoral inflammation, verified by histopathology of CD68+ and CD163+ cells in a rat orthotopic glioma model treated with an oncolytic herpes simplex virus, corresponds to the kinetics of MPO activity measured on excised brains through an enzymatic assay. These changes can be tracked in vivo through MPO-Gd-MRI. The specificity of the contrast induced by MPO-Gd was proved by comparing MPO-Gd-MRI with standard DTPA-Gd-MRI. Moreover, previously published works have shown that there is no detectable MPO-Gd-MRI contrast in mice knock-out for MPO, thus emphasizing the specificity of this MRI agent (26, 28, 31). The levels of viral LacZ and host MPO mRNAs display similar kinetics. However, whereas MPO mRNA is only detectable during the acute phase of this inflammatory response, a baseline of MPO activity is always present. This could be due to a general low abundance of MPO mRNA molecules or to a dual MPO regulation system: genetic and enzymatic (42). Because MPO-Gd-MRI is reproducible in mouse and rat gliomas established in the respective syngeneic animal model, and because we have shown that activation of CD68+ and CD163+ cells is not virus-, tumor-, or species-specific and that these cells infiltrate the tumor of patients treated with OV (19, 20, 22, 23) and secrete MPO, there is high translational potential for this technology. This is strengthened by the lower toxicity of MPO-Gd compared to many clinically-approved MRI agents (30).
An important advantage of MPO-Gd-MRI is its ability to distinguish between inflammation and tumor. While inflammation decreases between days 1 and 7 post viral dosing, the tumor size increases. Moreover, comparison of animals treated with two different doses of virus show stronger inflammation and smaller tumors for animals receiving the highest viral dose. Indeed, even though OV induce other oxidases in cancer cells, MPO-Gd is specific to MPO which is expressed only in myeloid cells. Current MRI strategies are not able to distinguish between inflammatory areas from tumor re-growth. This is a recurrent diagnostic dilemma that prevents the ability of the oncologists to provide the timeliest and most suitable treatment plan to the patient. Thus, this MRI technology can solve a critical diagnostic problem for the treatment of brain tumors. To establish the broad diagnostic applicability of this technology, it is important to test its capacity to detect inflammation during other therapeutic strategies such as radiation, immunotherapies, and treatment with anti-inflammatory and anti-angiogenic drugs.
Attempts to image intracerebral inflammation through MRI were previously done using MIONs (41), which detect all phagocytic cells. However, even though this strategy can detect OV-induced intratumoral macrophages (19, 20), it does not enhance the peritumoral inflammation, nor provides information on tumor size. Conversely, MPO-Gd-MRI can identify spatiotemporal changes of active inflammatory cells infiltrating into the cancer as well as in the brain parenchyma surrounding the tumor. Fusion of MION and MPO-Gd MRI scans in the same tumor model suggests that these two strategies detect three different cellular subsets: 1) intratumoral phagocytic cells not making MPO, 2) peritumoral MPO-secreting cells that are not phagocytic and 3) intratumoral phagocytic cells that also produce MPO. It is not clear if the peritumoral cells are not enhanced by MION-MRI because MIONs do not reach them or because they are not phagocytic. We have previously published that CD68+ microglia surrounding the tumor infiltrate into the tumor region and engulf the infectious OV (20), suggesting that MIONs do not diffuse to the peritumoral parenchyma. However, the phagocytic activity of these cells may be acquired only after their infiltration into the tumor, indicating that the different cellular subsets enhanced by MION and MPO-Gd-MRI are the same cells at different stages of inflammatory activation. Further comparison and combination of these imaging technologies will allow a deeper understanding of the distinct role of individual innate immune cells in the inflammatory responses (31, 39, 43–46).
Imaging inflammation is also useful in ways other than simply recognizing it in a re-occurring tumor after a specific treatment. As our understanding of cancer biology advances, increased relevance is being given to this host defense response. Even though the role of inflammation in the ultimate therapeutic outcome is unclear (being described both as controlling and promoting tumor recurrence and progression), it is accepted that it influences tumor treatment one way or another. It is therefore crucial to establish in vivo techniques that allow understanding of the relationship between inflammation and the outcome of tumor treatment. Demand for these techniques is further emphasized by the current trend of examining drugs that modulate immune processes (such as COX-2 inhibitors and NSAIDs) as anti-cancer agents. Finally, inflammation poses a crucial dilemma in OV-treatment. Even though it is established that host innate immunity is detrimental for OV lytic activity, inflammatory cells can also kill cancer cells and synergize with OV in tumor treatment (47, 48). Virotherapies aimed at increasing and suppressing OV-induced immunity were studied and both strategies presented positive results (47, 48). In this respect, our data indicate that increasing the viral dose, temporally augments also the infiltration/activation of MPO+ cells. Even though the higher viral dose transiently decreases the tumor size, it is impossible to establish from these data whether the temporal lysis of the tumor is mediated by OV or immune cells alone, or by the combination of these two factors. Further studies comparing MPO-Gd-MRI and MION-MRI during OV-treatment in presence of anti-inflammatory or pro-inflammatory agents will bring more insights into the role that different innate immune cells may have in the therapeutic outcome.
In conclusion, MPO-Gd MRI will strongly improve our diagnostic ability of the effects of cancer treatment on the tumor versus tumor micro-environment. Imaging inflammation during pro-inflammatory and immunosuppressive therapies will allow understanding of its role in cancer treatment and on side-effects of current therapies.
This work was supported by: the National Cancer Institute (R21-CA135526 to Giulia Fulci), the National Institute for Neurological Disorders (R01-NS070835, and R01-NS072167 to John Chen, R01-NS032677 to Robert Martuza, and P30-NS045776 to Samuel Rabkin), and the National Heart, Lung and Blood Institute (K08-HL081170 to John Chen) at the National Institutes of Health, USA.