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01.12.2017 | Research article | Ausgabe 1/2017 Open Access

BMC Cancer 1/2017

Methylene blue photodynamic therapy induces selective and massive cell death in human breast cancer cells

BMC Cancer > Ausgabe 1/2017
Ancély F. dos Santos, Letícia F. Terra, Rosangela A. M. Wailemann, Talita C. Oliveira, Vinícius de Morais Gomes, Marcela Franco Mineiro, Flávia Carla Meotti, Alexandre Bruni-Cardoso, Maurício S. Baptista, Leticia Labriola
Wichtige Hinweise

Electronic supplementary material

The online version of this article (doi:10.​1186/​s12885-017-3179-7) contains supplementary material, which is available to authorized users.
Singlet oxygen
Acridine orange
BCL2 and BCL2-associated X protein
B-Cell CLL/lymphoma 2
Band pass
Dulbecco’s Modified Eagle’s Medium/Nutrient F-12 Ham
Diethylene triamine penta acetic acid
Estrogen receptors
Reduced glutathione
Epidermal growth factor receptor-2
Hoechst 33342
High performance liquid chromatography
Light emitting diode
Long pass
Laser scan microscope
Lysosomal marker
Methylene blue
PDT Using methylene blue
Mitochondrial marker
Near infrared
Photodynamic therapy
Propidium iodide
Photon multiplier tube
Progesterone receptors
Polyvinyl difluoride
Roswell Park Memorial Institute Medium Modified
siRNA control of scrambled sequence
Triple-negative breast cancer


Breast cancer is a worldwide health problem for women, it is the first in incidence and the second in mortality among all cancer types, even with all recent technological advancements [ 1]. Early intervention is impactful, but a large number of patients still relapse even after years of apparent cure. The challenges in combating the disease relies on the intrinsic tumour resistance properties, molecular heterogeneity, and metastasis [ 13]. The molecular subtypes of breast cancers are defined based on the presence of oestrogen receptors (ER), progesterone receptors (PR), and human epidermal growth factor receptor-2 (HER2). About 20% of breast cancers are negative for ER, PR and HER2 expression (Triple-Negative Breast Cancer; TNBC) displaying aggressive pathological features and high rates of metastasis and recurrence [ 46]. For TNBC patients, the only current option is a non-targeted chemo and/or radiotherapy in order to extend the survival of patients, but does not reliably prevent a secondary disease [ 7].
Photodynamic therapy (PDT) is a promising alternative treatment for controlling malignant diseases [ 810]. PDT is based on the photooxidation of biological matter; the treatment involves the uptake of a photosensitizer (Ps) followed by illumination with light of an appropriate wavelength that is able to excite the Ps and trigger photochemical reactions that generate reactive oxygen species, such as singlet oxygen ( 1O 2), and radicals that lead to cell death [ 11]. The advantages of PDT compared with surgery, chemotherapy, or radiotherapy are the reduced long-term morbidity and the fact that PDT does not compromise other treatment options [ 11]. This therapy has been used as an experimental treatment modality in many countries for a number of cancers [ 12, 13]. In particular for non-superficial tumours, PDT appears promising in the treatment of high recurrence types of cancer. Indeed, it has been recently shown that PDT in combination with surgery in orthotopically implanted human pancreatic cancer in a nude mouse model was highly effective in eliminating microscopic disease in the post-surgical tumour bed as well as in preventing local and metastatic recurrence [ 14, 15].
For a variety of reasons, which include lack of studies on its efficacy and safety, as well as detailed mechanistic information, PDT is not a common type of treatment [ 12, 16, 17]. To overcome this scenario, many studies using PDT focus on the enhancement of Ps efficiency or in developing target-based PDT [ 18, 19]. However, because of the complexity of biological systems and unknown possible biological targets, details of how PDT operates are still elusive [ 13, 20]. Several approaches have also been developed using phenothiazinium derivatives, such as methylene blue (MB), as a new treatment strategy, leading to a PDT protocol which is efficient and also inexpensive [ 2125]. In addition to the low cost and commercial availability, the use of MB is also interesting because it has been safely used for decades in other clinical applications [ 21, 22, 26, 27].
In this study, we set out to explore the effectiveness of PDT using MB as Ps (MB-PDT) in different human breast cell lines, as well as the molecular mechanisms related to cell death. We demonstrated that MB-PDT is selective in inducing massive cell destruction of malignant cells, especially TNBC cells. We also observed that apoptosis is not the predominant route of cell death induced by MB-PDT. Finally, by using a tridimensional (3D) cell culture model, we confirmed the effectiveness of MB-PDT in selectively eliminating tumour cells while not affecting normal-like cells.


Cell cultures

Non-tumorigenic human MCF-10A (ATCC CRL-10317™) breast cell line was maintained in phenol red-free Dulbecco’s Modified Eagle’s Medium/Nutrient F-12 Ham (DMEM-F12; Sigma-Aldrich, St. Louis, MO, USA) supplemented with 5% heat-inactivated horse serum (Vitrocell Embriolife, Campinas, Sao Paulo, Brazil), insulin (10 μg/ml; Sigma-Aldrich), cortisol (500 ng/ml; Sigma-Aldrich), cholera enterotoxin (100 ng/ml; Sigma-Aldrich), and epidermal growth factor (20 ng/ml; Sigma-Aldrich). Human breast adenocarcinoma cell line MCF-7 (ATCC HTB-22™) was maintained in phenol red-free Dulbecco’s Modified Eagle’s Medium/Nutrient F-12 Ham (DMEM-F12; Sigma-Aldrich) supplemented with 10% heat-inactivated foetal bovine serum (FBS) (Vitrocell Embriolife). Human breast adenocarcinoma cell line MDA-MB-231 (ATCC HTB-26™) was cultured in phenol red-free Roswell Park Memorial Institute Medium Modified (RPMI 1640; Sigma-Aldrich) supplemented with 10% FBS (Vitrocell Embriolife). All cultures were maintained at 37 °C under water-saturated atmosphere containing 5% CO 2. For the 3D culture assays, (2x10 4/cm 2) cells were seeded on top of lamin-rich extracellular matrix gels (lrECM);commercially available as Matrigel (BD Biosciences, San Jose, CA, USA)- in phenol red-free medium supplemented with 2.5% serum and 5% lrECM and maintained for four days after treatments [ 28]. All 2D assays were also performed in 2.5% serum-supplemented medium.

Photodynamic treatment

Phenotiazonium salt, MB (Labsynth Products, São Paulo, Brazil) was used as Ps to perform the PDT treatment. Cells were incubated for 2 h with 0.2, 2 or 20 μM MB, in phenol red-free medium supplemented with 2.5% FBS and maintained in these conditions during both irradiation as well as post-treatment times (1, 3 and 24 h). The whole microplate was irradiated with a light emitting diode (LED) array, with maximum emission wavelength at 640 nm, corresponding to total light doses of 4.5 J/cm 2. Control experiments such as cells neither exposed to the Ps nor to light (control); cells not exposed to the Ps but washed and exposed to light (phototoxicity); and cells exposed to the Ps alone without irradiation (dark toxicity) were performed in all experiments.

Cell viability assay and morphological studies

4 × 10 4 cells/cm 2 were plated and maintained in control conditions or exposed to MB-PDT and then stained with the DNA-binding dyes Propidium iodide (PI, Sigma-Aldrich) and Hoechst 33342 (HO, Sigma-Aldrich) for 10 min. Following incubation, the percentage of viable and dead cells was determined using an inverted fluorescence microscope (Nikon Eclipse Ti, Kyoto, Japan) with 20x of magnification. Tri-dimensional cell cultures were transferred to a glass slide and visualized using a confocal microscope (Axiovert 200 LSM 510 Laser and Confocor Modules, Carl Zeiss, Göttingen, Germany) equipped with water immersion objective (40X). Fluorescence of labelled cells was detected using laser 461 nm and 545 nm for excitation of HO and PI respectively. The cultures were evaluated according to: the total number of cells, determined by counting the nuclei stained with HO; and the number of dead cells determined by the number of nuclei stained with PI or by brightly HO (condensed chromatin) [ 29]. A minimum of 500 cells was counted in each experimental condition. Results were expressed as percentage of dead cells.

Intracellular methylene blue quantification

1 × 10 5 cells/cm 2 were plated and incubated with 5 mL of medium containing MB (20 μM) and maintained for 1, 2, 4, 6 and 8 hours. At each time point, the supernatant was discarded and the cells were washed twice with PBS and then 1 mL of 50 mM SDS was added to promote lysis of the cell membrane. The supernatant was collected and absorbance was measured at the wavelength of maximum absorption of the MB solution used (655 nm). The incorporation of MB was determined by correcting the absorbance of MB by the number of cells remaining in each well after the incubation period.

Intracellular singlet oxygen generation

Singlet oxygen measurements were performed in a specially designed Edinburgh F900 instrument (Edinburgh, UK) consisted of a Rainbow OPO (Quantel Laser-France) 10Hz, 2 mJ/pulse, which was pumped by a Brilliant Nd-YAG laser (Quantel Laser-France) and equipped with a cuvette holder, a silicon filter, monochoromator, a liquid-nitrogen-cooled NIR PMT (R5509) (Hamamatsu Co., Bridgewater, NJ, USA) and a fast multiscaler analyser card with 5 ns/channel (MSA-300; Becker & Hickl, Berlin, Germany). The cells were seeded in six-well plates (4x10 5 cells/well) and after 24 h were incubated with MB for 2 h. The cells were washed in PBS, removed from the plates using trypsin solution, centrifuged and suspended in D 2O saline solution and were directly excited at 664 nm inside a fluorescence quartz cuvette. We obtained 1O 2 emission spectra by measuring emission intensities from 1200 to 1348 nm with 1 to 5 nm steps. The intensities of the near infrared (NIR) emission peak (centred at 1275 nm) are correlated with the amount of 1O 2 generated.

Glutathione quantification

Reduced glutathione (GSH) was quantified as previously described by Kand’ár et al [ 30] with minor modifications. Cells were seeded in Petri dishes (100 mm) at an initial density of 2.6 × 10 6 cells/Petri dish. After 48 h the cells were washed in PBS, removed from the plates using 0.1% trypsin, centrifuged and suspended in deionized water. An aliquot was separated for cell count before lysis with 0.15% polidocanol (Sigma-Aldrich). For protein precipitation, samples were incubated with cold 10% metaphosphoric acid (10 min, 4 °C), centrifuged (22,000 x g, 15 min, 4 °C) and supernatants were collected. The supernatant was diluted 20 folds in 100 mM phosphate buffer pH 8.9 containing 0.1 mM diethylene triamine pentaacetic acid (DTPA, Sigma-Aldrich). Twenty microliters of this sample were diluted to 320 μL in a 100 mM phosphate buffer pH 8.0 containing 0.1 mM DTPA. Derivatization was performed by adding 20 μL of 148 mM orthophthaldehyde (OPA, Sigma-Aldrich) to this solution. The reaction was incubated at 25 °C for 15 min in dark. The samples were then filtered through a 0.22 μm polyvinyl difluoride (PVDF) filter and injected onto high performance liquid chromatography (HPLC). The GS-OPA product was separated in a VP-ODS/C8/Phenyl column (250 mm × 4.6 mm × 4.6 μm, Shimadzu, Kyoto, Japan). The HPLC was equipped with two LC-20AT solvent delivery systems, SIL-20 AC HT autosampler, CTO-20HC column oven, RF-20A fluorescent detector and CBM-20A system controller (Shimadzu, Kyoto, Japan). The separation was achieved using an isocratic elution of 15% methanol in 85% 25 mM Na 2HPO 4 (Merck, Darmstadt, German) pH 6. The flow rate was constant at 0.5 mL/min 37 °C. Fluorescent GS-OPA was monitored with a ʎ ex 350 nm and ʎ em 420 nm. The peak area was plotted against an external GS-OPA standard curve previously derivatized with pure GSH (Sigma-Aldrich). Results were presented as pmol/cell.

Intracellular MB localization

We used confocal microscopy to characterize the subcellular localization of MB. To this end, we compared the fluorescence arising from cell cultures simultaneously incubated in the presence of MB and standard fluorescent markers of organelles. MitoTracker Green (Invitrogen, Paisley, UK) was used as a mitochondrial marker, LysoTracker Green (Invitrogen) as a lysosome marker and HO as a marker for the cell nucleus. Confocal images were taking using a laser scan microscope (LSM) - 510 from Zeiss using 1.2 N.A. 40x water immersion or 1.4 N.A. 63x oil immersion objective lenses. The laser and filter settings were: laser lines for MB = 633, Lyso = 488 and Hoechst 33342 = 364; beam splitter = HFT UV/488/543/633; emission filters for MB: 651-704, Lyso = 501-554 and Hoechst 33342 = 435-485. The imaging settings were: zoom = 1, dimensions = 512x512 pixels, image depth = 16 bit, averaging signal = 2 and optical section thickness = 2 μm. Images had their brightness and contrast adjusted for the figures and were analysed with ImageJ Software (National Institutes of Health).

Detection of acidic vesicles in live cells using acridine orange

Acridine orange (AO) is a weak base that can accumulate in acidic spaces and emits bright red fluorescence. The intensity of the red fluorescence is proportional to the pH of the cellular acidic compartments [ 31]. In order to detect and quantify acidic vesicle formation during the process of autophagy, 4x10 4 cells/cm 2 were plated and then subjected or not to MB-PDT. Cells were then washed with PBS and stained with AO (Sigma Aldrich) at a final concentration of 5 μg/ml for 10 min at 37 °C in the dark. After a washing step, live cells were visualized using an inverted microscope for transmitted light and epifluorescence (Axiovert 200, Carl Zeiss) equipped with a C-APOCHROMAT 40×/1.20 M27 objective (Zeiss™). Fluorescence of AO-stained vesicles was detected by using a filter set 09 (Zeiss™) that provides an excitation band pass (BP) of 450-490 nm with emission long pass (LP) of 515 nm.

Inhibition of signaling pathways

4.0 × 10 4 cells/cm 2 were plated and incubated with each inhibitor in the presence or in the absence of MB for 2 h, in a 5% CO 2 humidified atmosphere at 37 °C. Cells were then subjected or not to light irradiation as described above. Apoptosis was inhibited by using a specific caspase-3 inhibitor (100 nM Caspase-3 Inhibitor VI; Calbiochem, La Jolla, CA, USA), a pan-caspase inhibitor (20 μM Z-VAD-FMK; Calbiochem) or a BAX inhibitor (10 μM; Tocris, Ellisville, MO, USA). Autophagy was activated using mTOR inhibitor rapamycin (20 nM; Cell Signaling Technology, Danvers, MA, USA) or inhibited by using either PI3-kinase inhibitor LY294002 (50 μM; Tocris), class III PI3K inhibitor 3-MA (5 mM; Calbiochem), chloroquine (5 μM; Sigma-Aldrich) or bafilomycin A1 (50 nM; Calbiochem). We analysed the dose-response and toxicity of each inhibitor and we used the highest concentration that presented no cytotoxicity in the control conditions for each cell line.

Transient oligonucleotide transfection

The siRNA used in this study was a Silencer pre-designed siRNA (Invitrogen) of sequence 5’GCUCUGCCUUGGAACAUCAtt 3’. “AllStars negative control siRNA” (Qiagen, Venlo, Netherlands) was used as a negative siRNA control of scrambled sequence (siCTR). Transfection of siRNA was done using the lipid carrier Lipofectamine RNAiMAX (Invitrogen). Lipid-RNA complexes were formed in Opti-MEM (Invitrogen) in a proportion of 0.6 μl of Lipofectamine to 0.45 μl of 20 μM siRNA, at room temperature for 20 min and were further added to cells in antibiotic-free medium to reach a final volume of 300 μl for overnight transfection. Cells were maintained in culture for a 24-h recovery period before experiments were carried out. The efficiency of transfection/silencing was validated by Western blot, with at least 60% of inhibition.

Western blots

Total protein extracts were prepared from each culture subjected to the treatments described above. Equal amounts (100 μg) of protein from each extract were solubilized in sample buffer (60 mM Tris-HCl [pH 6.8], 2% SDS, 10% glycerol, 0.01% bromophenol blue) and subjected to SDS-PAGE (16%). Proteins were transferred to PVDF membranes, incubated with Blocking Buffer solution (Thermo Fisher Scientific) and 5%BSA 1:1, and then incubated with the following antibodies: rabbit polyclonal anti-BAX (2772), rabbit polyclonal anti-BCL2 (2876) (all from Cell Signaling Technology), rabbit polyclonal anti-LC3 (L8918) and mouse monoclonal anti-alpha-tubulin clone B-5-1-2 antibody (T5168) (all from Sigma-Aldrich) as a loading control. Membranes were then incubated with horseradish peroxidase-conjugated secondary antibody (Vector Laboratories, Burlingame, CA, USA). Enhanced chemiluminescence was performed according to the manufacturer’s instructions (Amersham Biosciences, Little Chalfont, UK). Quantitative densitometry was carried out using the ImageJ software (National Institute of Health [NIH]). The volume density of the chemiluminescent bands was calculated as integrated optical density × mm 2 after background correction.

Caspase-3, caspase-7, caspase-8 and caspase-9 activity assays

4 × 10 6 cells were collected and caspase activity was measured using a specific fluorimetric assay (BioVision Research Products, Mountain View, CA, USA). The reactions were started at 37 °C by incubating 50 μg of total protein extracts with a specific caspase substrate (50 μM DEVD-AFC, 50 μM IETD-AFC or 50 μM LEHD-AFC for caspase-3 and -7; -8 and -9, respectively; BioVision), following the manufacturer’s instructions. Protease activity was evaluated at an excitation wavelength of 400 nm and an emission wavelength of 505 nm using a 96-well plate spectrofluorometer (Spectra MAX M2; Molecular Devices, Sunnyvale, CA, USA). Total protein extracts from Min6 cells exposed to either vehicle or a combination of pro-inflammatory cytokines which induced a significant and well documented degree of apoptosis [ 3235], were always included as a positive control for caspase-3, -7, -8 and -9 activity assays, in each experiment performed. Caspase-3, -7, -8 and -9 activities were expressed as arbitrary fluorescence units per 50 μg of total protein (At least 3 independent experiments were performed in triplicate for each condition).

Statistical analysis

All results were analysed for Gaussian distribution and passed the normality test. The statistical differences between group means were tested by One-way ANOVA followed by Tukey post-test for multiple comparisons. A value of p < 0.05 was considered as statistically significant.


MB-PDT selectively induces cell death in breast cancer cells, whereas not significantly affecting non-malignant cells

Taking into account the heterogeneity of the most common breast cancer types and also to test the possible cytotoxic effects of MB-PDT in normal-like cells, we used the following human breast epithelial cell lines: MCF-7, an ER, PR and HER-2-positive, luminal A cell line; MDA-MB-231, a TNBC cell line; and MCF-10A, a normal-like cell line. Figure  1 (a and b) shows time curves of cell death after MB-PDT with 2 or 20 μM MB followed by irradiation with 4.5 J/cm 2. The treatment consistently had a higher impact in the malignant cell lines and presented a maximal effect 24 h after irradiation in the presence of 20 μM MB. The TNBC cells showed the highest rate of cell death (24 h: 98.6% ± 0.5%), followed by MCF-7 cells (93.0 ± 5.2%) and then by the normal-like MCF-10A cells (52.2% ± 3.8%). Additionally, unlike the exponential increase in cell death over time presented by the other cell lines, in the presence of the highest MB concentration, MDA-MB-231 cells reached the maximal percentage of photodynamic destruction at earlier time points (1 h).
Using the lower concentration of MB, we detected that the normal-like cells were even less sensitive to MB-PDT (24 h: 18.0% ± 7.2%). It is important to note that this dose still induced massive death in the malignant cell lines at the same time point (MDA-MB-231: 97.3% ± 0.7% and MCF-7: 78.3% ± 7.1%). These data allowed us to establish a window of time for our mechanistic studies. It is important to note that cells submitted to irradiation alone (without MB) or MB alone up to 24 h of incubation (to test dark toxicity) showed no significant differences in cell death in comparison to untreated cells. Moreover, survival of all cell lines exposed to different MB concentrations or light alone was similar to the values obtained for the negative control conditions (see Additional file 1: Figure S1).
To analyse whether the distinct susceptibility to MB-PDT was due to differences in MB uptake, we measured the intracellular levels of MB and observed no statistical differences in the Ps content among all cell lines (Fig.  1c). We also assessed 1O 2 generation capability and detected similar levels of this oxidant molecule between all cell lines (Fig.  1d). These results led us to conclude that the lower effect of MB-PDT was neither due to intracellular concentrations of the Ps nor to the amount of intracellular singlet oxygen. To evaluate if there was any differential stress-adaptive response to MB-PDT, we measured intracellular glutathione and found lower reduced glutathione (GSH) levels in MDA-MB-231 cells (Fig.  1e). This indicates that glutathione-dependent stress-control mechanism might be important to determine the sensitivity to the prooxidant milieu generated by MB-PDT.

Relevance of apoptosis in MB-PDT-induced cell death

We analysed the typical morphological changes related to cell death in the nuclei after treatment. MB-PDT did not induce neither the pyknotic and fragmented nuclei or condensation of chromatin into small, irregular and circumscribed patches, typical patterns of apoptotic cells in any time point or MB concentration tested (Fig.  2a, and see Additional file 1: Figure S2). As a control for typical apoptotic nuclei morphology, MDA-MB-231 cells were treated with the known apoptotic inducer staurosporine [ 36, 37]. The differences between typical morphology of nuclei undergoing apoptosis displayed by staurosporine-treated cells and the one displayed in MD-PDT-treated cells, led us to hypothesize that MB-PDT induced death through a non-apoptotic route.
However, according to the current classification of cell death subroutes, only the presence of specific morphological features is not sufficient to establish which mechanism is mediating cell deletion [ 38, 39]. Thus, we also evaluated biochemical hallmarks of apoptosis. We analysed viability curves upon MB-PDT in the presence of either Z-VAD-FMK, a pan-caspase inhibitor, or of a specific caspase-3 inhibitor (Fig.  2b). Strikingly, our results demonstrated that both inhibitors exerted a cytoprotective effect at initial times after MB-PDT, but failed to completely prevent cell death in malignant cells. We also assessed the activity of initiator caspases-8 and -9, as well as executioner caspase-3 and -7 (Fig.  3). Corroborating the inhibition assays, no caspase-3 involvement was detected in MB-PDT-induced cell death in either MCF-10A or MCF-7 cells. However, a significant transient peak of caspase-8 activity was observed at initial times after MB-PDT in MDA-MB-231 cells and in MCF-10A cells at 24 h after treatment.
These results led us to propose that a caspase-independent apoptotic pathway could mediate MB-PDT-induced cell deletion. Therefore, to further determine the relevance of the apoptosis pathway after MB-PDT, we evaluated the balance between anti- and pro-apoptotic proteins of the B-Cell CLL/lymphoma 2 (BCL2) family. As shown in Fig.  4a, none of the experimental conditions tested induced a decrease in BCL2 and BCL2-associated X protein (BAX) protein ratio. We also tested the effect of a BAX specific inhibitor on MB-PDT efficiency (Fig.  4b). Cell viability revealed that the inhibition of BAX pore formation is harmful for all cell lines, which can then become more susceptible to MB-PDT. Altogether these data presented evidence that the caspase-independent apoptotic pathway had no relevance in MB-PDT-induced cell damage.

MB fluorescence concentrates at the lysosomes of breast cancer cells

To determine the subcellular localization of MB in organelles involved in cell death mechanisms, we incubated the cells with MB in combination with a nuclear marker and either a lysosomal (LysoTG) or a mitochondrial marker (MitoTG). All cell lines showed some level of colocalization of LysoTG and MB fluorescence signals. However, in the MDA-MB-231 cells, MB was highly concentrated at the lysosomes showing a near perfect overlap with LysoTG staining (Fig.  5 and see Additional file 1: Figure S3a). In sharp contrast, this pattern of colocalization was not observed for MB and MitoTG (see Additional file 1: Figure S3b). This finding represents a preferential lysosomal localization of MB, which makes this subcellular compartment prone to photochemistry damage induced by MB-PDT instead of the mitochondrion or the nucleus.

MB-PDT-induced autophagy leads to an increase in cytoprotection only in MDA-MB-231 and MCF-10A

A large number of different cell types initiate autophagy following photoirradiation [ 40]. Our results showed an increase in acidic structures already at early time points after MB-PDT in MDA-MB-231 cells (Fig.  6a). Moreover, a significant increase in LC3-II/LC3-I ratio was observed not only upon MB-PDT, but also after irradiation or MB incubation controls alone (Fig.  6b). In MDA-MB-231 cells, autophagosome formation was higher at initial times after PDT with 2 μM MB. These data showed autophagy was induced by the treatment, but it did not appear to be related to cell death. To determine whether the role of autophagy in MB-PDT is a mechanism of death or an attempt to rescue damaged cells, we assessed viability after MB-PDT by inhibiting or inducing autophagy. MDA-MB-231 and MCF-10A cells displayed a significant cell death increase upon autophagy inhibition with all inhibitors tested (Fig.  6c). In contrast, the autophagic flux induced by rapamycin decreased cell death in MDA-MB-231 and MCF-10A cells exposed to MB-PDT. This effect was not observed in MCF-7 cells, where an autophagy induction even resulted in increased cell susceptibility to MB-PDT. Consistent with these results, autophagy silencing by siRNA-mediated knockdown of ATG5 confirmed that this pathway elicits a cytoprotective role in MDA-MB-231 and MCF-10A but not in MCF-7 cells (Fig.  6d). In conclusion, our results indicated that autophagy might be related to an initial pro-survival response of the cells to the oxidative damage generated by MB-PDT in TNBC and normal-like cells, but not in luminal A cells.

Spheroid culture enhances the differential sensitivity to MB-PDT of malignant and normal-like cells

In order to validate our results in a model that recapitulates the morphology of glandular epithelium, we compared the different responses in cells cultured on plastic surfaces (2D monolayers) or on top of a commercial basement membrane (3D). When cultured in a 3D environment, breast epithelial cells form multicellular structures; the normal-like cells organize into polarized, growth-arrested acini containing a lumen, whereas malignant cells form overgrown and disorganized tumour-like masses [ 28] (Fig.  7a). Thus, this strategy provides a more physiologically relevant assay to analyse the effect of treatments against malignant cells.
The same MB-PDT photocytotoxicity protocol used for cells grown on monolayers was performed in 3D cultures. Dose response curves using 20 μM MB followed by irradiation with 4.5 J/cm 2 showed that there was no obvious cell viability inhibition both at 1 and 3 h after MB-PDT treatment. However, cell death was significantly increased after 24 h of PDT for both breast cancer cell lines (MDA-MB-231: 87.1% ± 1.8%; MCF-7: 74.4% ± 1.5%) (Fig.  7b). Importantly, MB-PDT effect in cancer cells cultured in 3D after 24 h did not differ significantly from the effect observed in 2D after MB-PDT, but normal-like cells cultured in 3D displayed a significantly lower sensitivity to the treatment than those cultured in 2D (Fig.  7c).


In this study we have demonstrated that MB-PDT induced massive cell death in two human breast cancer cell lines displaying different invasive properties. The highest sensitivity to MB-PDT was observed in MDA-MB-231 cells, used as a model of TNBC, a tumour subtype for which there are no targeted treatments. This effect is very relevant because TNBC tumours are the greatest challenge in breast cancer treatment nowadays [ 7]. With MB-PDT, we obtained almost 100% of cell death in these malignant cells. Our results are significantly better than the ones obtained in other reports using PDT for treating breast cancer cells [ 10, 4143]. Other Ps used in previous studies, such as Mitoxantrone, present dark toxicity, which is not desired for PDT practice [ 12, 16]. In our study using MB we observed no dark toxicity, a feature which can increase local specificity and safety of the treatment.
One of the advantages of PDT over other cancer treatments is the possibility of generating less side effects to patients [ 810]. Our results demonstrated the efficacy of MB-PDT in selectively eliminating breast cancer cells. Among the few reports found in literature, Shemesh and collaborators have recently showed a small difference of only 20% in cell death between MFC-10A and MDA-MB-231 cells submitted to liposomal Indocyanine green-PDT [ 44]. In the present work, we have reached a difference of up to 80% of MB-PDT-induced cell death between malignant and normal-like cells.
Since it has already been demonstrated that MB is a classical 1O 2 generator [ 45], we compared parameters like oxidative potential and antioxidative capability between the cell lines. The photodynamic action of MB leads to the production of similar levels of 1O 2 in the intracellular microenvironment, so that is not a limitation for MB-PDT efficiency. As a prooxidant therapy, PDT is able to cause the collapse of antioxidant systems, leading to cell death [ 19]. Among the systems involved in the homeostasis of the intracellular redox balance, glutathione plays a major role [ 46]. It has been reported that TNBC cells present lower GSH levels compared to ER positive cells [ 47]; furthermore, cell lines containing low GSH levels tend to be much more sensitive to cancer therapies [ 46]. In this study we confirmed that TNBC cells present the lowest GSH intracellular levels among the studied cell lines, and that this could be related to the inability of these cells to cope with MB-PDT-induced oxidative stress. This result pointed MB-PDT as a potential strategy to effectively kill malignant cells that lack specific therapeutic targets by impacting metabolic properties that differ from those found in normal tissues.
There are few in vitro systematic studies on the molecular mechanisms induced by PDT that compare both malignant and normal-like mammary cells. These reports demonstrated that apoptosis is the main cell death pathway activated by PDT [ 4851]. Nevertheless, we argue that in these studies classical characteristics of apoptosis have not been observed after PDT. Therefore, we hypothesize that apoptosis may not be the predominant process that mediates cell death induced by PDT, but only a by-product of other activated mechanisms [ 22]. Other authors also stated that the predominant type of cell death depends on the protocol adopted, and that there may be variations from apoptosis to necrosis depending, for example, on the energy dose used [ 11]. In our study we observed no presence of apoptotic traits under any dose, treatment time, or irradiation intensity used. Additionally, cell viability was not completely restored with the use of caspase inhibitors. Furthermore, MB-PDT action could not be exerted exclusively by apoptosis because MCF-7 cells do not express caspase-3 [ 52]. Additionally, no increase in caspase-7, -8 or -9 activities was detected in MCF-7 cells upon MB-PDT. In this context, we also observed no decrease in the ratio of anti- and pro-apoptotic proteins and that inhibition of the mitochondrial pore formation increased the sensitivity of the cells to MB-PDT, pointing to a probable mitochondrial-independent cell death pathway. Reinforcing this hypothesis, we showed that MB is not localized or, as already reported, it may be in a reduced state in mitochondria [ 45], thus strongly suggesting that this organelle is indeed not the primary target for MB-PDT oxidative damage.
Depending on a network of signals generated at specific cellular sites, cells can respond differentially to stress [ 53]. Previous studies exploring the subcellular localization of MB indicated that this Ps presents a tendency to accumulate in lysosomes of living cells [ 45]. We reported here for the first time evidence of differential patterns of lysosomes and MB colocalization in different epithelial cell lines of the same tissue. In view of the organelle-specific initiation of cell death, this data may contribute to explain the differential cellular sensitivity to MB-PDT observed among the three analysed cell lines.
The data on the lysosomal localization of MB, led us to explore the involvement of autophagy in the context of MB-PDT. The relationship between autophagy and cell death in PDT is still extensively discussed in the literature. Some studies pointed this pathway as responsible for the cell damage generated by different Ps [ 54, 55]. Others have shown that this type of cell death only occurs upon prevention of classical apoptosis, such as a result of mutations in essential apoptotic-related genes such as BCL2 or caspase family members [ 40, 56]. Our data showed an intensification of the autophagic pathway upon MB-PDT which lead either to cytoprotection or cytotoxicity in a cell-dependent manner. This is expected since MCF-7 cells are haploinsufficient for Beclin-1 [ 57], which could be the reason for their increased sensitivity for MB-PDT.
The fact that cancer cells can die through different mechanisms is a relevant clue in the choice and design of anticancer therapies based on molecular targets [ 55]. We have found that, depending on the cell type, multiple cell death pathways might be activated upon MB-PDT. Indeed, we showed that apoptosis and autophagy are related, but not the main cell death inducing pathways. Moreover, preliminary results from our group are pointing some of the regulated necrosis pathways (i.e. necroptosis) as more relevant mechanisms involved in MB-PDT-induced cell death (data not shown). Since one important aspect for an alternative therapy for cancer treatment is to broaden the spectrum of cell death mechanisms to by-pass the different resistance mechanisms displayed by malignant cells, we are at the present time focusing our resources to further dissect the alternative molecular pathways leading to MB-PDT photocytotoxicity.
From an oncological point of view it is of fundamental importance if a therapy can achieve the ultimate goal of eliminating tumour cells, despite the complexity of the tumour microenvironment [ 58]. 3D cultures allows for the reestablishment of biochemical and morphological characteristics that resemble the conditions of the cells in their in vivo environment [ 28]. Since 3D cultures present the advantage of the formation of microenvironments and differential exposure to distinct factors such as nutrients and oxygen, this approach represents a robust model for the study of incorporation and bioactivity of drugs [ 59]. Moreover, it has been shown that 3D assays can be used successfully to effectively distinguish malignant and normal tissue responses to therapy [ 28, 60]. We have demonstrated that MB is efficiently incorporated in the complex gelatinous matrix used for the 3D cell cultures; it is able to enter the 3D structures and to be photoactivated inducing cell death isotropically throughout the spheroids. Our results indicate that in this model MB-PDT was also effective in inducing cell destruction of cancer cells, with an even higher selectivity between tumours and normal-like cells. This enhancement in MB-PDT preferential response in tumour cells might be due to the protective effect exerted by the organized basement membrane and tissue polarity seen in the acini formed by MCF-10A cells [ 61, 62].
In sum, MB-PDT holds promise as a useful adjunct to surgery to eliminate microscopic residual malignant cells in the post-surgical tumour bed and prevent local as well as metastatic recurrence without affecting normal tissues. In particular for breast cancer, PDT is not currently being tested as a peri-opertive therapy like the one described for pancreatic cancer (14-15); however, all results presented in this work pointed us the importance to pursue further studies in this direction in a near future. The strategy could be of particular importance in TNBC because metastatic recurrence after surgical tumour resection is a major and frequent cause of patient mortality.


When compared to other studies of PDT on breast cancer, we have reached a greater efficiency in selectively killing cancer cells with no MB dark cytotoxicity. Besides, we demonstrated the differential effect of MB-PDT in more than one cell line, overcoming an important caveat in many PDT studies that use either only one tumour cell line or cell lines from different tissues. To the best of our knowledge, we have also shown for the first time that normal-like cells of breast epithelium are much more resistant to MB-PDT. These are fundamental features for the safe usage of the therapy, reinforcing the fact that one of the advantages of PDT over other therapeutic approaches is the possibility of generating fewer side effects to the patients. Finally, we propose that MB-PDT could be an effective and safe adjunct to surgery leading to lower rates of local and distant recurrence.


We are grateful for the fundamental assistance provided by Luciana Rodrigues Gomes (Department of Microbiology, Institute of Biomedical Sciences, University of São Paulo, São Paulo, Brazil).


This work was supported by FAPESP (grants 12/16785-4, 13/07029-4, 12/50680-5 and 13/07937-8), CAPES, CNPq (grant 141529/2012-1) and by the NAP-PhotoTech-USP. The funding agencies only financially supported this study. They did not participate in either the design of the study, collection, analysis and interpretation of data or in writing the manuscript.

Availability of data and materials

All data supporting our findings can be found in the main paper or in the additional supporting files.

Authors’ contributions

AFS, LFT, MSB and LL contributed to the conception and experimental design of the study, data analysis and interpretation of the results. AFS carried out most of the experiments. LFT, RAMW, TCO, VMG, MFM and ABC performed some experimental work. FCM helped with GSH quantification experiments and analysis. ABC helped with microscopy data acquisition and analysis. AFS and LL wrote the manuscript. AFS, MSB and LL are responsible for the integrity of the work as a whole. All authors revised the article and approved the final version to be published.

Authors’ information

AFS, RAMW, TCO, VMG and MFM are University of São Paulo PhD students; LFT is a University of São Paulo post-doc; ABC, FCM and LL are University of São Paulo assistant professors; MSB is a University of São Paulo full professor.

Competing interests

The authors declare that they have no competing interests.

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Not applicable.

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Additional file 1: Figure S1. MB-PDT induced massive cell death in MDA-MB-231 without dark cytotoxicity. (a) Representative graph showing the viability of MCF-10A, MCF-7 and MDA-MB-231 cells after MB-PDT with 20 μM of MB followed by 4.5 J/cm2 irradiation and the experimental controls: irradiation alone (λ); dark toxicity of MB, that means incubation without irradiation (MB); or not treated cells (control). These results were obtained after 24 h (n = 3 independent experiments); *: p < 0.05 versus control. (b) Viability of MDA-MB-231 cells after MB-PDT with MB (20 μM) followed by 4.5 J/cm2 or 1.5 J/cm2 irradiation after 24 h. Results are shown as mean ± s.e.m. (n = 3 independent experiments); *: p < 0.05 versus 4.5 J/cm2. Figure S2. MB is preferentially localized in the lysosomes. (a) Low magnification images of the data shown in Fig. 5 of the cells simultaneously incubated with LysoTracker green (LysoTG) and MB. Merged images of the following two images (yellow; left column). MB Fluorescence (red; middle column) and fluorescence arising from LysoTracker (green; right column). (b) Confocal microscopy images of the cells simultaneously incubated with MitoTracker green (MitoTG) and MB. Merged images of the following two images (yellow; left column). MB Fluorescence (red; middle column) and fluorescence arising from MitoTracker (green; right column). Hoechst 33342, indicating nuclei. [MB] = 20 μM; [LysoTG] = 300 nM; [MitoTG] = 300 nM; nucleus (HO 3334 = 300 nM). Size bar: 10μm. Figure S3. No evidences of apoptotic nuclei after MB-PDT. (a) Representative nuclei of human mammary cells treated for 1 h, 3 h and 24 h with MB-PDT with 0.2 μM of MB. Nucleus stained with Hoechst 33342 (blue) and propidium iodide (red). Size bar: 20μm (b) Viability time curves after MB-PDT of cell cultures with 2 (a) or 20 μM of MB (b) followed by of 4.5 J/cm2 irradiation obtained after 1 h, 3 h and 24 h post-irradiation (n = 3 independent experiments) * p < 0.05 versus MCF-10A. Results are shown as mean ± s.e.m. (DOCX 2074 kb)
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