Comparison of the killing effects between nitrogen-doped and pure TiO2 on HeLa cells with visible light irradiation
© Li et al.; licensee Springer. 2013
Received: 14 December 2012
Accepted: 29 January 2013
Published: 22 February 2013
The killing effect of nitrogen-doped titanium dioxide (N-TiO2) nanoparticles on human cervical carcinoma (HeLa) cells by visible light photodynamic therapy (PDT) was higher than that of TiO2 nanoparticles. To study the mechanism of the killing effect, the reactive oxygen species produced by the visible-light-activated N-TiO2 and pure-TiO2 were evaluated and compared. The changes of the cellular parameters, such as the mitochondrial membrane potential (MMP), intracellular Ca2+, and nitrogen monoxide (NO) concentrations after PDT were measured and compared for N-TiO2- and TiO2-treated HeLa cells. The N-TiO2 resulted in more loss of MMP and higher increase of Ca2+ and NO in HeLa cells than pure TiO2. The cell morphology changes with time were also examined by a confocal microscope. The cells incubated with N-TiO2 exhibited serious distortion and membrane breakage at 60 min after the PDT.
KeywordsNitrogen-doped TiO2 Visible-light-activated Photodynamic therapy Reactive oxygen species
In recent years, semiconductor titanium dioxide (TiO2) was noticed as a potential photosensitizer in the field of photodynamic therapy (PDT) due to its low toxicity, high stability, excellent biocompatibility, and photoreactivity [1–4]. The electrons in the valence band of TiO2 can be excited to the conduction band by ultraviolet (UV) radiation with the wavelength shorter than 387 nm (corresponding to 3.2 eV as the band gap energy of anatase TiO2), thus resulting in the photoinduced hole-electron pairs. These photoinduced electrons and holes can interact with surrounding H2O or O2 molecules and generate various reactive oxygen species (ROS, such as superoxide anion radical O2 ·−, hydroxyl radical OH · , singlet oxygen 1O2, and hydrogen peroxide H2O2), which can react with biological molecules, such as lipids, proteins, and DNA, cause their damages, and eventually kill cancer cells [1, 9, 10].
However, the pure TiO2 can only be excited by UV light which is harmful and hinders its practical applications . Fortunately, recent studies have reported that the optical absorption of TiO2 in the visible region could be improved by doping [12–14] or dye-adsorbed methods [15, 16], which will facilitate the application of TiO2 as a photosensitizer for PDT. In our previous study , we enhanced the visible light absorption of TiO2 by nitrogen doping and found that the nitrogen-doped TiO2 (N-TiO2) showed much higher visible-light-induced photokilling effects on cancer cells than the pure TiO2.
Although great efforts have been made to prepare doped TiO2 with visible light absorption, the underlying mechanism of the killing effects of photoactivated TiO2 on cancer cells has not yet been investigated in details. It is unclear how the TiO2 interacts with the cancer cells, and what are the differences for their photokilling effects between pure and doped TiO2. For possible medical applications of N-TiO2, it is of crucial importance to understand the killing effect of N-TiO2 on cancer cells and the mechanism of cell damages induced by PDT.
As ROS has been claimed to be of major importance for various kinds of PDT [17–20], the time-dependent ROS productions during visible light irradiation were evaluated in this work for both N-TiO2 and TiO2 in aqueous suspensions. The productions of different ROS species, such as O2 ·−, H2O2, and OH·, were also studied. Furthermore, a systematic comparison of the intracellular parameters with N-TiO2 and TiO2 nanoparticles as photosensitizers for PDT was investigated. The changes of mitochondrial membrane potential (MMP), intracellular Ca2+, and nitrogen monoxide (NO) concentrations with time after the PDT were measured. The relationships between these parameters were discussed. The morphological changes of cytoskeletons after irradiation were also examined by a confocal microscope at different times after the PDT. The killing effects between pure and nitrogen-doped TiO2 were compared.
Preparation and characterization of N-TiO2 samples
The details of preparation of N-TiO2 nanoparticles were described in our previous paper . Briefly, The anatase TiO2 nanoparticles (particle size <25 nm; Sigma-Aldrich, St. Louis, MO, USA) were calcined at a flow rate of 3.5 L/min in ammonia atmosphere at 550°C for 20 min to produce the N-TiO2 nanoparticles. The crystalline phases of the N-TiO2 nanoparticles were determined by Raman spectra to be anatase. The ultraviolet-visible (UV/Vis) diffuse reflectance absorption spectra (Additional file 1: Figure S1) of the N-TiO2 and TiO2 samples were measured with a Jasco V550 UV/Vis spectrophotometer (Jasco, Inc., Tokyo, Japan).
Pure and N-doped TiO2 nanoparticles were autoclaved and dispersed in DMEM-H medium at a concentration of 100 μg/ml, respectively. The samples were ultrasonicated for 15 min before using.
Cell culture and PDT treatment
The human cervical carcinoma cells (HeLa) procured from the Cell Bank of Shanghai Science Academy were grown in Petri dishes in DMEM-H solution supplemented with 10% fetal calf serum in a fully humidified incubator at 37°C with 5% CO2 for 24 h.
The cells were incubated with 100 μg/ml pure or N-doped TiO2 under light-free conditions for 2 h and were then illuminated with a visible light filtered by a bandpass filter (400 to 440 nm) from a Xe lamp (100-W; Olympus, Center Valley, PA, USA) at a power density of 40 mW/cm2 for 5 min. The transmission spectrum of that bandpass filter was shown in Additional file 2: Figure S2. As shown in the figure, the filter could transmit some light with the wavelength below 400 nm. Therefore, the pure TiO2 could still absorb a small amount of the transmitted light.
Measurement of ROS induced by TiO2 or N-TiO2 in aqueous suspensions
For the measurement of photo-induced ROS in TiO2 or N-TiO2 aqueous suspensions, 2′,7′-dichlorfluorescein (DCFH), was used as a probe. The DCFH was converted from the diacetate form DCFH (DCFH-DA) (Sigma-Aldrich) by adding 0.5 ml of 1 mM DCFH-DA in methanol into 2 ml of 0.01 N NaOH and keeping the mixture at room temperature in the dark for 30 min. It was then neutralized with 10 ml sodium phosphate buffer (pH = 7.2) . Pure or N-doped TiO2 in phosphate buffered saline (PBS, 100 μg/ml) were mixed with DCFH (25 μM) before visible light irradiation. The non-fluorescent DCFH can rapidly react with ROS to form fluorescent 2′,7′-dichlorofluorescein (DCF). By measuring the fluorescent intensity, the production of ROS could be estimated.
To measure the generations of specific ROS, two probes were used respectively. Dihydrorhodamine 123 (DHR) is mainly sensitive to O2 ·− and H2O2, and 2-[6-(4-aminophenoxy)-3-oxo-3H-xanthen-9-yl]-benzoic acid (APF) is selectively sensitive to OH · . It was already demonstrated that the reactive species H2O2, O2 ·−, and 1O2 did not cause any modification in the fluorescence of the probe APF . Pure or N-doped TiO2 in PBS (100 μg/ml) were mixed with DHR (25 μM, Sigma-Aldrich) or APF (10 μM, Cayman Chemical, Ann Arbor, MI, USA) before irradiation. Upon oxidation, the non-fluorescent DHR or APF is converted to the highly fluorescent Rhodamine 123 or fluorescein.
After the samples were irradiated by a visible light (400 to 440 nm) with a power density of 40 mW/cm2 for different times ranging from 1 to 5 min, the fluorescence spectra were recorded by a spectrometer (F-2500, Hitachi, Brisbane, CA, USA) and the fluorescent intensities were compared.
Rhodamine 123 [2-(6-amino-3-imino-3H-xanthen-9-yl) benzoic acid methyl ester] (Beyotime, Jiangsu, China), which could bind specifically to the mitochondria, was used to estimate the MMP. When MMP is decreased, the dye could be released from the mitochondria and the fluorescence vanished. The PDT-treated cells were incubated with Rhodamine 123 (5 μg/ml) for 30 min in the dark at 37°C and then were washed with Dulbecco’s PBS (D-PBS) for three times before the visible light illumination.
Measurement of Ca2+ concentration
To study the intracellular calcium concentration, HeLa cells were loaded with 10 μM Fluo-3 AM (Beyotime) for 30 min at 37°C and followed by washing with D-PBS for three times. Then the cells were incubated for another 20 min to ensure complete cleavage of Fluo-3 AM by the intracellular ester enzyme that releases Fluo-3 before the illumination.
Measurement of intracellular NO
The intracellular NO level was detected using a NO-sensitive fluorescence probe DAF-FM DA [3-amino, 4-aminomethyl-2′,7′-difluorescein, diacetate] (Beyotime). The cells were loaded with 10 μM DAF-FM DA at 37°C in the kit buffer for 20 min and were then gently washed with D-PBS for three times and incubated for another 20 min to ensure that the intracellular DAF-FM DA was completely catalyzed to form DAF-FM by ester enzyme before the illumination.
Cell morphology and cytoskeleton observation
The HeLa cells were fixed with 4% paraformaldehyde for 15 min at room temperature with different time intervals after the illumination. Then they were permeabilized with 0.025% Triton X-100 in D-PBS (Sigma-Aldrich Corp., St. Louis, MO, USA) for 2 min. After washing with D-PBS three times, the cells were treated with 1% bovine serum albumin (BSA) for 2 h at 4°C. The fixed cells were stained with 5 nM Alexa Fluor® 488 phalloidin conjugate (Invitrogen, Eugene, OR, USA) for F-actin labeling for 40 min at 37°C. Meanwhile, 1% BSA was added to the staining solution to reduce nonspecific background staining. The cells were washed with 0.05% PBS-Tween20 three times before microscopic observation.
Microscopy and image analysis
The fluorescence images of cells were observed by a laser scanning confocal microscope (FV-300, IX71; Olympus, Tokyo, Japan) using a 488-nm continuous wave Ar+ laser (Melles Griot, Carlsbad, CA, USA) as the excitation source and a × 60 water objective to focus the laser beam. A 505- to 550-nm bandpass filter was used for the fluorescence images. Each experiment was repeated three times independently.
The fluorescence intensities of MMP, Ca2+, and NO probes from the microscopic images were analyzed with the Olympus Fluoview software. The data were expressed in terms of the relative fluorescence intensity of the probes and expressed as mean ± SD. The fluorescence intensity was averaged from 100 to 150 cells for each experiment.
Results and discussion
Generation of ROS by pure and N-doped TiO2 in aqueous suspensions
OH · is mainly formed in the reaction of photogenerated holes with surrounding water, while O2 ·− is formed in the reaction of photogenerated electrons with dissolved oxygen molecules. Some O2 ·− can form 1O2 by reacting with the holes. Moreover, some OH · can form H2O2, and the reactions of H2O2 can also result in the formation of OH · with a lesser extent.
Since DCFH is a nonspecific ROS probe, it is necessary to further analyze the specific ROS. As described above, DHR and APF were used to evaluate the generation of O2 ·−/H2O2 and OH·, respectively. The fluorescence measurements in Figure 1b,c shows that all the specific ROS increased with the irradiation time, but the N-TiO2 induced more O2 ·−/H2O2 (Figure 1b) while less OH · (Figure 1c) than TiO2. It was reported that the photogenerated holes of N-TiO2 were trapped in the N 2p levels and had a very low mobility , thus were barely involved in the photocatalysis when the N-TiO2 was illuminated by visible light . In this study, the lower production of OH · from N-TiO2 might result from the same reason. However, the photogenerated electrons in the conduction band can react with oxygen molecules to generate O2 ·−, which is thermodynamically favored . Thus, N-TiO2 could generate more O2 ·−/H2O2 than the pure TiO2 due to the higher visible light absorption efficiency.
When cells were treated with TiO2 or N-TiO2 nanoparticles, the nanoparticles were not only found on the cell membrane but also in the cytoplasm, and some of them aggregated around or in Golgi complexes and even in nuclei . As the TiO2 or N-TiO2 nanoparticles can induce ROS under visible light irradiation, the photokilling effect on cancer cells was observed in our previous work . Considering that the productions of the specific ROS species generated by TiO2 or N-TiO2 are different and the contributions from the specific ROS to PDT may also be different, the PDT-induced changes of the intracellular parameters, such as MMP, Ca2+, and NO concentrations in HeLa cells treated with TiO2 or N-TiO2 were studied as follows.
It should be noted that the MMP level of N-TiO2-treated cells decreased 3.5 times faster than that of the TiO2-treated cells at the beginning after the PDT. Compared with Figure 1c that there were considerably more OH · induced by TiO2 than N-TiO2 under visible light, it strongly suggested that the hydroxyl radicals with the rather shorter lifetime and lower diffusion length than O2 ·− and H2O2 might contribute less on the damage of mitochondria among a variety of ROS in PDT.
Intracellular Ca2+ concentration
It has been reported that some signal transduction pathways were activated by PDT . Calcium expression level was one of the concerning principal factor since it is an important link between the pathways. The activation of Ca2+ was also known as a contributor to the cell morphological and functional changes associated with apoptosis . The raise of intracellular calcium levels would result in various changes of cellular metabolism as well as the cell morphology.
As shown in Figure 3, the Ca2+ levels for both TiO2 and N-TiO2 samples reached the maximum values at about 45 min after the PDT, where N-TiO2 induced release of Ca2+ at around 2.1-fold than TiO2 did. Since there was no calcium ion in the D-PBS solution, the detected Ca2+ might be released from the damaged calcium stores, such as mitochondria and possibly other organelles, and flow into the cytoplasm through ion channels .
This result agreed with the data of MMP changes. The MMP levels of N-TiO2 decreased around 3.5 times faster than that of TiO2 at the early time after the PDT, which means the N-TiO2 induced damage of mitochondria was more serious. Therefore, the released Ca2+ could be observed earlier and the Ca2+ levels were higher in N-TiO2 samples as compared to the TiO2 samples.
Generation of NO
Cell morphology and cytoskeleton defects
As ROS can be generated around TiO2 or N-TiO2, the nanoparticles near the cell membranes may directly cause cell membrane damage by biochemical reactions. Additionally, the PDT-induced defect of mitochondria and the release of Ca2+ into the cytoplasm might trigger cell apoptosis or necrosis, which may result in the cell morphology and cytoskeleton defects eventually. As the cytoskeleton is involved in many intracellular signaling pathways, the cytoskeletal distortion and shrinkage need to be further studied for a long observation time in future studies.
A comparison of the killing effects between N-TiO2 and TiO2 on HeLa cells with visible light irradiation was conducted. N-TiO2 produced more ROS and specifically more O2 ·−/H2O2 under visible light irradiation. Contrarily, more OH · were produced by TiO2. The MMP levels were sensitive in the PDT, and rapid loss of MMP was detected at the very beginning after the PDT as one of the earliest detectable biochemical changes in this study. A certain amount of MMP loss (around 24%) was followed by the detectable increase of Ca2+ (at 5 and 15 min after the PDT for N-TiO2 and TiO2, respectively). The increase of NO was detected later than the other intracellular parameters, which indicates that the NO generation was caused by the generation of ROS. The N-TiO2 resulted in more loss of MMP and higher increase of Ca2+ and NO in HeLa cells and, finally, induced more cell damages than pure TiO2. At 60 min after irradiation, significant cytoskeletal shrinkage and breakage were observed for N-TiO2-treated cells, whereas for TiO2-treated cells, only slight damage was demonstrated. Overall, N-TiO2 can induce more cell damages than pure TiO2. The hydroxyl radicals might contribute less to the cell damages among a variety of ROS.
This work is supported by the National Natural Science Foundation of China (61008055, 11074053), the Ph.D. Programs Foundation of Ministry of Education of China (20100071120029), and the Key Subjects Innovative Talents Training Program of Fudan University.
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