Background
Osteosarcoma (OS) is a malignant aggressive primary bone tumor that commonly arises in the long bones of children and young adults. Conventional clinical treatment consists of surgical resection of the tumor and adjuvant chemotherapy [
1]. In spite of the effort made by clinicians in the last 30 years, the success of OS treatment is limited to a 70% 5-years survival rate with the remaining 30% of OS patients not responding to standard treatments [
2] mainly because of the formation of lung metastases, which ultimately represent the primary cause of mortality [
3]. Despite testing different drugs and regimens, a substantial improvement of survival rate has not been observed [
4‐
6]. In addition to lung metastases, OS cells resistance to chemotherapeutics, such as doxorubicin [
7], greatly hampers treatments’ efficacy, therefore the development of innovative and more selective strategies capable of improving the survival of OS patients is required.
Mesenchymal stromal cells (MSCs) have been proved to be powerful tools in cell therapy, being used for a wide array of clinical indications spanning from the treatment of graft-versus-host-disease to tissue engineering, and currently are tested in several hundreds of clinical trials [
8]. Additionally, thanks to their proven ability to migrate and engraft in the stroma of several tumors [
9], MSCs have been used in preclinical and clinical studies as carriers of antitumor drugs with the aim of enhancing their selective accumulation at the tumor site. In 2002, Studeny et al. firstly proposed MSCs as carrier cells for gene therapy [
10]; at present, several studies have been published reporting MSCs as effective delivery vehicles of anticancer agents, such as pro-apoptotic molecules, chemotherapeutic drugs and oncolytic viruses [
11‐
20]. In addition, it has been extensively demonstrated that MSCs can internalize and deliver nanoparticles loaded with therapeutic agents [
21‐
25], including chemotherapeutic drugs and photosensitizers (PS) for photodynamic therapy (PDT) applications [
26‐
28].
In PDT, light at a specific wavelength is applied to the tumor site where the PS localizes after administration; once irradiated, the PS enters an excited state that triggers the formation of various reactive oxygen species (ROS) responsible for killing cancer cells and the damage of tumor vasculature that in turn deprives the tumor of oxygen and nutrients [
29]. In particular, the use of nanoparticles as PS delivery systems has been proposed as treatment for several tumors with the aim of bypassing biological barriers and cellular chemo-resistance [
30]. PDT has proved to be a successful, clinically approved, and minimally invasive alternative/co-adjuvant therapeutic option to conventional therapies for the treatment of various tumors [
31,
32]. In particular, PDT has been proved to be effective in decreasing tumor growth both in in vitro and in vivo OS models [
33‐
40], and in a murine model of aggressive prostate tumor [
41] as well as in clinical settings [
42].
In order to establish whether the PDT driven MSCs strategy is an effective system for the treatment of OS, we designed a multistep process that could allow us to determine the best operating settings, such as: doses, radiant exposure and distance of light source, time after infusion of loaded MSCs, safety of the operating procedure etc., with in mind the possibility of clinical translation. With this in mind, in an earlier study we demonstrated that MSCs can be efficiently and safely loaded with fluorescently labelled poly-methyl methacrylate nanoparticles (FNPs) electrostatically decorated with the photosensitizer tetra-phenyl sulfonated porphyrin (TPPS), and that this system (TTPS@FNP@MSCs) exerts a ROS-mediated cytotoxic effect on surrounding OS cells upon irradiation with a 405 nm light in-vitro [
26]. Based on these encouraging results, we improved our NPs system by loading a different PS, i.e. tetra-sulfonated aluminum phthalocyanine (AlPcS
4), since it is well-established that the optimal light therapeutic window, ensuring the highest tissues penetration, falls in the near-infrared region [
43]. In fact, unlike TPPS, AlPcS
4 has a strong absorption peak in the near-infrared region of the spectrum; this upgraded system, i.e. AlPcS
4@FNPs, was able to effectively kill human prostate cancer cells in in vitro 3D model as well as in in vivo mouse model [
41].
Therefore, the objective of the current study is to prove whether our AlPcS4@FNPs particles are an effective PDT system against OS cells; more importantly, we aim to investigate in an in vivo OS ectopic model whether AlPcS4@FNPs loaded into MSCs have an improved tumor selectivity compared to AlPcS4@FNPs alone, while maintaining their cancer cells killing efficacy.
Material and methods
Reagents
Dulbecco’s Modified Eagle’s Medium-high glucose (DMEM-HG, glucose 4500 mg/L), McCoy’s medium, and Ficoll®-Paque PREMIUM 1.073 reagents were purchased by Sigma Aldrich (Saint Luis, Missouri, USA). α-Minimum Essential Medium Eagle (α-MEM) was purchased by Lonza (Verviers, Belgium). Fetal Bovine Serum (FBS), GlutaMAX, penicillin/streptomycin solution, Dulbecco’s phosphate buffered solution without calcium and magnesium (D-PBS), Puromycin, Alexa Fluor® 488 Annexin V/PI Dead Cell Apoptosis Kit, LIVE/DEAD® Viability/Cytotoxicity Kit (Calcein-AM and Ethidium homodimer-1), Alamar Blue, and WST-1 assay reagents were purchased from Thermo Fisher Scientific (Waltham, Massachusetts, USA). CellTiter-GLO® was purchased from Promega (Milano, Italy). Tetra-sulfonated aluminum phthalocyanine (AlPcS4) was purchased from LivChem Logistics GmbH (Frankfurt, Germany).
Preparation of AlPcS4@NPs/FNPs
Poly-methyl methacrylate (PMMA) core-shell fluorescent nanoparticles (FNPs) were obtained by an emulsion-co-polymerization reaction as previously described [
26,
41]. Briefly, 2-(dimethyloctyl)-ammonium ethyl-methacrylate bromide (0.52 g, 1.5 mmol) in water (50 mL) was placed into a 250 mL three-necked reactor equipped with a mechanical stirrer, a condenser, a thermometer and a nitrogen inlet. The mixture was heated to 80 °C under stirring (300 rpm), and 2-aminoethyl methacrylate hydrochloride (AEMA, 0.25 g, 1.48 mmol) was added to the solution. Afterward, a mixture of allyl 2-(3-allyloxy-6-oxo-6H-xanthen-9-yl) benzoate [
44] (0.003 g, 0.007 mmol) and methyl methacrylate (0.93 mL, 9.35 mmol) was added to the previously obtained solution. After 10 min, 15 mg (0.05 mmol) of 2,2′-azobis (2-methylpropionamidine) dihydrochloride (AIBA), dissolved in 0.5 mL of mQ water was added to the mixture, which was then allowed to react for 4 h. The reaction product was purified by dialysis (against water) to remove residual monomer and stabilizer. Whenever needed, and to avoid interference with fluorescent staining, non-fluorescent PMMA nanoparticles (NPs) were prepared by the same procedure without the addition of the fluorescent comonomer, i.e. allyl 2-(3-allyloxy-6-oxo-6H-xanthen-9-yl) benzoate AlPcS
4@FNPs or AlPcS
4@NPs stock solution was prepared by adding 50 μl of AlPcS
4 (1 mg/mL in milliQ water) to 50 μl of FNPs or NPs (10 mg/mL) and milliQ water to a final 1 mL volume. The stock solution was diluted in complete cell culture medium to the desired concentration. Where not explicitly stated, the indicated concentrations refer to the amount of FNPs/NPs per volume unit, resulting in an equivalent AlPcS
4 concentration of 1/10 (e.g. 90 μg/ml AlPcS
4@FNPs are equivalent to 9 μg/mL AlPcS
4).
Human osteosarcoma cell lines
Human osteosarcoma cell lines, MG-63 (CRL-1427), Saos-2 (HTB-85) and U-2 OS (HTB-96) were purchased from ATCC (Manassas, Virginia, USA). Briefly, cells were cultured respectively in DMEM-HG (MG-63) or McCoy’s medium (Saos-2, U-2 OS) containing 10% of FBS, 1% GlutaMAX and 50 U/ml penicillin/streptomycin at 37 °C in a humidified atmosphere with 5% CO2.
Saos-2-Luc/GFP cell line was generated by transduction with Lentivirus particles containing the CMV promoter for the expression of humanized firefly luciferase (hLUC) and SV40 promoter for the expression of GFP protein according to manufacturer’s protocol (GeneCopoeia). Three days after infection, cells with high levels of GFP expression were selected by Cell Sorter NIR Aria II (BD Bioscience) and expanded for a week in culture medium supplied with Puromycin to generate a stable cell line.
Isolation and culture of human mesenchymal stromal cells (MSCs)
MSCs were obtained from bone marrow samples of five patients undergoing surgery at Rizzoli Orthopedic Institute (Bologna, Italy). Isolation and culture expansion of human MSCs was performed as previously described in Pierini et al. [
45] with minor modifications. Briefly, mononucleated cells were isolated from bone marrow through gradient separation with Ficoll®-Paque PREMIUM 1.073, then placed in 150 cm
2 culture flasks in complete growth medium (αMEM+ 20% FBS) at a density of 4 × 10
5 cells/cm
2 and incubated at 37 °C in 5% CO
2 atmosphere. Medium was changed every 3–4 days; after the first passage sub-culturing was performed at 2 × 10
3 cell/cm
2 every time the cells reached a 70–80% confluence. Complete characterization in terms of fibroblast-colony forming unit (CFU-F) efficiency, immunophenotypic profile, proliferation rate, and trilineage-differentiation potential of each MSC line was performed. Since ex-vivo expanded MSCs are a heterogeneous population and are known to be highly sensitive to the protocols used to isolate and expand the cells in culture [
46,
47], detailed protocols are provided as Supplementary Methods (Additional file
1), and all MSCs’ characterization and in-process data are provided for review in Table 1S (Additional file
2), as suggested by Reger and Prockop [
48]. In order to account for unpredictable variations on test results due to the well-known donor-to-donor variability of MSCs [
49], at least 3 different MSCs lines were tested in independent experiments. When stated, all the 5 MSCs lines were tested, in order to strengthen the reproducibility of the results. Only cells from the third to the sixth passage were used in all experiments.
Cytotoxicity assay
MSCs were seeded in 96 well plates and incubated for 1 h with AlPcS4@FNPs, FNPs or AlPcS4 at increasing doses (45, 90, 180 μg/mL for AlPcS4@FNPs or 4.5, 9, 18 μg/mL for AlPcS4). Cells were then washed twice with D-PBS and new complete medium was added to each well. WST-1 assay was performed 1, 2 and 6 days after loading following the manufacturer’s instructions. The optical density of each well was measured by a microplate reader (Synergy HT, BioTek Winooski, VT, USA) set at 450 nm with the correction wavelength set at 690 nm.
MSCs loading with nanoparticles
MSCs were seeded at 104 cells/cm2 in complete medium and allowed to adhere to the plates overnight before loading. MSCs were exposed to AlPcS4@FNPs or AlPcS4@NPs diluted in complete medium for 1 h, then washed two times with D-PBS. AlPcS4@FNPs or AlPcS4@NPs loaded MSCs were allowed to recover for a time varying from 2 h to overnight (o/n) in complete medium, before being detached from culture flasks, for subsequent experiments. Before each experiment, AlPcS4@FNPs loaded MSCs were checked through automated cell counter Countess II® FL (Thermo Scientific, Waltham, Massachusetts, USA) in order to verify the loading efficiency.
Cellular uptake and accumulation
The percentage of loaded MSCs were determined by BD FACScanto II cytometer (Becton-Dickinson, Franklin Lakes, NJ, USA) and by the automated cell counter Countess II® FL (Thermo Scientific, Waltham, Massachusetts, USA), taking advantage of FITC fluorescence of FNPs. For confocal microscopy (Nikon, Amsterdam, Netherlands) analysis, MSCs were seeded onto glass coverslips, loaded with FNPs and at the indicated time points fixed for 10 min in 10% Neutral Buffered Formalin at room temperature, thoroughly washed with D-PBS, stained with Hoechst and imaged.
In vitro migration study
Cell migration was assessed by the Boyden chamber technique. Cell culture inserts for 24-well plate with 8 μm pore diameter were used (Millipore, Darmstadt, Germany). After a recovery period of 2 h in complete medium, AlPcS4@FNPs loaded MSCs, along with unloaded MSCs used as control, were exposed to o/n starvation, switching the complete medium to αMEM+ 0.2%FBS. Then 104 cells were placed in the upper chamber in 200 μL of αMEM+ 0.2%BSA. Six hundred microliters of αMEM supplemented with 20% FBS (chemo-attractant) or 0.2% BSA (neutral) was added into the lower chamber. After overnight incubation, cells on the upper face of the membrane were removed with a cotton swab while the ones on the bottom surface were fixed in 100% methanol and stained with Hema-stain kit (Fischer Scientific, Hampton, New Hampshire, USA). Cells migrated through the microporous membrane were counted in 10 randomly chosen fields under an inverted Nikon Eclipse TE2000-U microscope (Nikon, Amsterdam, The Netherlands).
2D co-culture
MSCs were loaded with 90 μg/ml AlPcS4@FNPs and left o/n to recover in complete medium. AlPcS4@FNPs loaded MSCs were then trypsinized, counted with Countess II® FL and 5 × 103 cells were seeded into 24-well plate mixed with 5 × 103 or 15 × 103 Saos-2 cells, i.e 1:1 or 1:3 ratio respectively. Photoirradiation was delivered after overnight cell adhesion.
3D co-culture
MSCs were loaded with 90 μg/ml AlPcS4@FNPs and left for a recovery period of 4 h in complete medium. AlPcS4@FNPs loaded MSCs were then trypsinized, counted and mixed with MG-63 in different ratios (1:1, 1:3 and 1:7) to a final concentration of 105 mixed cells/mL in DMEM-HG + 10%FBS. One hundred microliters aliquots of the suspension were dispensed in an ultra-low attachment U-bottom 96-well plate (Corning Costar, Amsterdam, The Nederlands) and allowed to aggregate for 4 days to form regularly shaped spheroids.
Photodynamic therapy parameters
In in vitro experiments, AlPcS4@NPs loaded MSCs were photoactivated using a LED light source (λmax = 668 ± 3 nm) at room temperature, with the light-emitting unit placed directly under the tissue culture plates (radiant power: 140 mW). Monolayer cultures (2D) received photoactivation for 5 min, while spheroids (3D) for 10 min. Viability assays were performed, in all experiments, 24 h after PDT treatment.
In in vivo model, the tumor bearing area was irradiated for 20 min using the same LED source but with the addition of a focusing device (i.e. a cylinder of 0.6 cm diameter and 2 cm length, with a light-reflecting internal surface). The end of the focusing device was placed in close proximity to the mouse skin (Radiant power: 130 mW). Treatment was repeated twice, once a week.
Cell viability assays
In 2D co-culture, cell death was evaluated by Alexa Fluor® 488 Annexin V/Propidium Iodide Dead Cell Apoptosis Kit according to the manufacturer’s protocol and analyzed with BD FACScanto II cytometer (Becton-Dickinson, Franklin Lakes, NJ, USA). Cell survival rate was determined by Alamar blue assay following the manufacturer’s instructions. The fluorescence of each well was measured by a microplate reader (Synergy HT, BioTek Winooski, VT, USA) with excitation/emission wavelengths of 530/590 nm. The fluorescence intensity from the samples was corrected using a cell-free control as blank.
For 3D co-culture system, cell death was evaluated through the ATP content–based assay CellTiter-Glo® 3D following the manufacturer’s protocol. Additionally, a LIVE/DEAD® staining was performed. Spheroids were incubated with 2.5 μM Calcein-AM in DMEM Phenol Red-free for 2 h, then Ethidium homodimer-1 (EthD-1) was added to a 5 μM final concentration for 10 min. Z-stacks images, for a total depth of 100-120 μm, were acquired with an A1R confocal laser scanner (Nikon, Amsterdam, The Netherlands) using Nikon Plan Apo VC 20x/0.75 NA DIC N2 objective lens and 3D rendering was performed with NIS elements software using the Alpha-blending algorithm.
Transmission electron microscopy (TEM)
Spheroids were fixed with 2.5% glutaraldehyde in 0.1 M cacodylate pH 7.6 buffer for 1 h at room temperature. After post-fixation with 1% OsO4 in cacodylate buffer for 1 h, cells were dehydrated in an ethanol series and embedded in Epon resin. Semithin sections of 0.8 μm were cut using an ultramicrotome and stained with toluidine blue. Ultrathin sections (70 nm) were contrasted with uranyl acetate and lead citrate and observed with a Jeol Jem-1011 transmission electron microscope (Jeol Jem, USA).
Animal study
Eighteen female Athymic-nude mice, aged 6–8 weeks, were subcutaneously injected into the left flank with a mixture of Saos-2/Luc cells (1 × 106) and MSCs (1 × 106) in 50 μL of PBS/Matrigel. When tumors reached 100–150 mm3, approximately 2 weeks post-injection, the mice were divided into four groups: two control groups (group I and II respectively PBS and AlPcS4), group III AlPcS4@FNPs alone and group IV AlPcS4@FNPs loaded into MSCs. Fifty microliters of PBS, AlPcS4 (9 μg/mL), AlPcS4@FNPs (90 μg/mL) and AlPcS4@FNPs loaded-MSCs (1 × 106) were intra-tumorally injected. The next day, the mice were exposed for 20 min to PDT. Intra-tumor injection and PDT treatment were performed weekly for 2 weeks. All animals were euthanized 1 week after the last treatment. After intra-tumor administration of test substances, the whole animal fluorescent imaging (excitation/emission wavelengths: 640/680 nm) was performed using the IVIS Lumina II (PerkinElmer, Waltham, MA) to observe AlPcS4@FNP nanoparticles biodistribution. The same instrumentation was used to monitor tumor growth through bioluminescence imaging (BLI). D-luciferin (GolBio, St Louis, MO) dissolved in PBS (1.5 mg luciferin/100 μL PBS) was injected intraperitoneally at a dose of 150 mg D-luciferin/kg. The BLI imaging was performed prior NPs/NPs loaded MSCs injections and after PDT treatment. Regions of interest (ROIs) were drawn within the tumor to measure average radiance (expressed as photons/s/cm2/sr) using Living Image® 4.2 software (Caliper Life Sciences, Hopkinton, MA).
Histology
Tumors were collected, fixed in 4% paraformaldehyde solution, and embedded in paraffin. Samples were sectioned at a thickness of 4 μm and hematoxylin and eosin (H&E) staining was performed for a general inspection of the pathologic specimens. To evaluate the extent of tumor apoptosis and validate the BLI results, a terminal deoxynucleotidyl transferase dUTP nick end labeling (TUNEL) assay was performed with a commercial kit (Roche, Mannheim, Germany). Ki-67 staining for cell proliferation was also performed. Images of tumor tissue were taken by a NIKON Upright BF&Fluorescent light microscope.
Statistical analysis
All results were obtained from at least three independent experiments and expressed as the mean ± SD. Two-way ANOVA followed by Dunnett’s multiple comparisons test was used to determine statistical probabilities in the in vivo results. Results were considered to be statistically significant at P-values < 0.05. The statistical analysis was processed with GraphPad Prism 6 Software (GraphPad; San Diego, CA, USA).
Discussion
Despite the effort made by clinicians in the last 30 years, 30% of osteosarcoma (OS) patients still do not respond to standard treatments, succumbing to the disease [
50]. Major issues for poor OS survival rate include the insurgence of distal metastases [
51,
52], mainly localized in the lungs, and the development of multi drug resistance (MDR) [
53,
54]. Possible strategies for improving OS patients’ survival rate include methods for selectively targeting the therapeutic agent to the tumor stroma, as well as the use of alternative therapeutic approaches able to either circumvent MDR or kill chemoresistant cells.
In this context, mesenchymal stromal cells (MSCs) are increasingly considered as an ideal vector for delivering antineoplastic drugs, because of their well-established ability to home towards the stroma of several primary and metastatic tumors [
55,
56]. Indeed, MSCs have been used for the in vitro and in vivo delivery of, among others, diagnostic and therapeutic agents, small interfering RNA and nanoparticles [
57]. In particular, several authors have shown that MSCs easily internalize different types of nanoparticles [
27] and can reach the tumor, showing limited or no toxicity effect of NPs to MSCs [
58,
59]. Additionally, other authors have investigated whether MSCs can transport nanoparticles for therapeutic purposes [
22,
60,
61].
Among alternative cancer treatments, photodynamic therapy (PDT) has been successfully used to kill OS cells in vitro [
35,
37,
62‐
65]; in particular Kusuzaki et al. has shown that PDT is also able to kill multidrug resistant OS cells [
66]. In vivo the effectiveness of PDT has been demonstrated in OS animal models [
34,
67,
68]. Moreover, PDT has been previously successfully used to treat sarcomas in a group of patients in which PDT inhibits the local recurrence after intralesional tumor resection [
38,
69‐
71].
Our results successfully demonstrate that the internalization of AlPcS
4@FNPs into MSCs takes place in 1 h, and that particles are retained in the cells for at least 3 days. This result is in line with Roger et al. work, where they demonstrated that PLA nanoparticles are internalized by MSCs up to 100% within 1 h, and that the particles are retained for at least 3 days [
23,
24]. This aspect is particularly significant in view of clinical application since a 3 days interval is compatible with the migration of MSCs to the tumor from the site of the injection [
72].
The awareness recently acquired that a monolayer culture is not predictive of in vivo results, prompted us to find an ex vivo model able to simulate in vivo physiology [
73]. Tumor spheroids are an established model to investigate novel cancer treatments, as they provide a better recapitulation of tumor pathophysiological aspects, such as the in vivo-like differentiation pattern due to the appropriate 3D extracellular matrix (ECM) assembly and the complex cell–matrix and cell–cell interactions [
74,
75]. Particularly, in our case the thickness of the cell aggregate (~ 400 μm of diameter), together with the presence of extracellular matrix and the inevitable oxygen gradient, provided a more challenging model for the PDT treatment. In this model, we clearly demonstrated that the efficacy of the photoactivation of AlPcS
4@FNPs loaded MSCs depends on the ratio between MSCs and OS cells. As expected, this result suggested that the in vivo efficacy of this system will strongly depend on both the tumor’s dimensions and on the number of loaded MSCs that will reach the neoplastic region.
Additionally, by combining the results obtained from the APT content analysis, the Live&Dead staining assay and the TEM microscopy studies, we were able to establish that by decreasing the MSCs:OS ratio from 1:1 to 1:7, cell death is far higher in the center of the spheroid as respect to the outer region. This observation could be explained by the outgrowth of OS cells in the 4 days of spheroids formation that would ultimately confine MSCs in the more internal part of the spheroid. A similar distribution of MSCs in a spheroid model has been observed by Zhang et al. in melanoma cell spheroids [
25].
As a starting point to test the efficacy in vivo of AlPcS4@FNPs loaded MSCs, an ectopic OS model was developed. An arbitrary dose of MSCs loaded with AlPcS4@FNPs was selected and injected intra-tumorally and the efficacy of two photoactivation cycles was tested. Compared to the control groups (PBS and AlPcS4 alone), after the second photoirradiation, tumor growth was reduced in both groups (AlPcS4@FNPs and AlPcS4@FNPs@MSCs, 72 and 68% respectively). Results observed by luminescence analysis were confirmed by histological changes in the treated tumor sections. Clear evidence of apoptosis, observed by H&E and TUNEL staining, were associated with PDT treatment in combination with AlPcS4@FNPs injection (alone or loaded in MSCs), supporting the role of our system in the cell-killing process after photoirradiation.
The results described herein demonstrate that the AlPcS
4@FNPs@MSCs system is very promising for treating OS tumors. However, treatment outcome could be improved by increasing PDT efficacy, by either performing more irradiation cycles or/and by optimizing the AlPcS
4@FNPs loaded MSCs dose as well the irradiation conditions. Importantly, even if a reduction of tumor growth was demonstrated in both groups of mice, i.e. AlPcS
4@FNPs alone and AlPcS
4@FNPs@MSCs, in the mice injected with AlPcS
4@FNPs alone, the NPs had a larger distribution as shown in Fig.
5a, thus supporting the tumor targeting effect of MSCs. Furthermore, it is interesting to notice that only mice injected with AlPcS
4@FNPs alone, displayed skin superficial burns, probably generated by an excessive local heating due to an over-concentration of the particles in the skin and their subsequent photoactivation, as already observed by others [
76]. This data further supports the potential advantage of using MSCs as a delivery system in terms of selective localization at the target tissue, which in turn allows the control of unwanted side effects.
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