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This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Neuroblastoma, a frequently occurring solid tumour in children, remains a therapeutic challenge as existing imaging tools are inadequate for proper and accurate diagnosis, resulting in treatment failures. Nanoparticles have recently been introduced to the field of cancer research and promise remarkable improvements in diagnostics, targeting and drug delivery. Among these nanoparticles, quantum dots (QDs) are highly appealing due to their manipulatable surfaces, yielding multifunctional QDs applicable in different biological models. The biocompatibility of these QDs, however, remains questionable.
We show here that QD surface modifications with N-acetylcysteine (NAC) alter QD physical and biological properties. In human neuroblastoma (SH-SY5Y) cells, NAC modified QDs were internalized to a lesser extent and were less cytotoxic than unmodified QDs. Cytotoxicity was correlated with Fas upregulation on the surface of treated cells. Alongside the increased expression of Fas, QD treated cells had increased membrane lipid peroxidation, as measured by the fluorescent BODIPY-C11 dye. Moreover, peroxidized lipids were detected at the mitochondrial level, contributing to the impairment of mitochondrial functions as shown by the MTT reduction assay and imaged with confocal microscopy using the fluorescent JC-1 dye.
QD core and surface compositions, as well as QD stability, all influence nanoparticle internalization and the consequent cytotoxicity. Cadmium telluride QD-induced toxicity involves the upregulation of the Fas receptor and lipid peroxidation, leading to impaired neuroblastoma cell functions. Further improvements of nanoparticles and our understanding of the underlying mechanisms of QD-toxicity are critical for the development of new nanotherapeutics or diagnostics in nano-oncology.
Neuroblastoma is the most frequently occurring extracranial solid tumour in children, accounting for 9% of all childhood cancers, with poor prognosis . This malignant tumour arises from neuroepithelial cells of the sympathetic nervous system early in development, and is typically found in the adrenal medulla, abdomen, chest or neck . Neuroblastoma, however, remains a therapeutic challenge as current surgical and chemical treatments are insufficient to prevent tumour recurrence, metastasis and progression . Accurate disease staging is critical for appropriate therapeutic intervention, but existing imaging tools are still lacking in early and accurate diagnosis .
The introduction of nanoparticles in the field of cancer research has recently improved diagnosis, targeting and drug delivery with the use of nanotubes, liposomes, dendrimers and polymers [5-7]. Other nanoparticles, such as quantum dots, possess excellent photophysical properties and prove to be an elegant alternative to the traditional bioimaging tools . Quantum dots (QDs) are one of the most rapidly evolving products of nanotechnology, with great potential as a tool for biomedical and bioanalytical imaging. Their superior photophysical properties  and sometimes multifunctional surfaces are suitable for applications in various biological models . A study by the Nie group describes the application of these multifunctional QDs for in vivo imaging and targeting of breast and prostate cancers . Although the development of QDs as bioimaging tools may be well underway, their potential application as therapeutic agents is yet to be explored. Biological media, intracellular microenvironment and different enzymatic systems could destabilize originally well protected QD surfaces yielding more cytotoxic nanoparticles [12,13]. Uncoated or weakly stabilized cadmium telluride QDs produce significant amounts of reactive oxygen species in vitro , and induce death in various cell types [14,15].
Oxidative stress-induced cell death, both apoptosis and necrosis, can involve a number of cellular mechanisms, one of which includes the activation of Fas receptor [16,17]. Fas (CD95) belongs to the family of tumour necrosis factor receptors, and is a prototypical "death receptor." In the immune system, it regulates cell numbers by inducing apoptosis, and is involved in T cell-mediated cytotoxicity. It can also induce neuronal cell death [18-21]. Activation of Fas receptor by Fas ligand recruits the Fas-Associated Death Domain (FADD) to the Death Domain in the cytoplasmic tail of the receptor, and can lead to caspase activation and cell death . Downstream signaling of Fas can also induce activation of lipases and pro-apoptotic transcription factors like p53, which then potentiate apoptosis .
Oxidative stress can also induce other levels of cell membrane damage, including membrane lipid peroxidation . Free radicals induce the cleavage of membrane lipids, resulting in the production of aldehydes, reinforcing cellular stress. Intracellular lipid peroxidation can also occur at the level of the organelle membranes, especially at the membranes of the highly metabolically active mitochondria. Mitochondria regulate crucial cellular processes including adenosine triphosphate (ATP) production, intracellular pH regulation and neuronal-glial interactions . Many neurodegenerative diseases, including Parkinson's and Alzheimer's diseases, involve the malfunctioning of the mitochondria, seen as decreased mitochondrial activity, decreased ATP production or loss of mitochondrial membrane potential (Δψm) .
In this study, we explored mechanisms of QD-induced toxicity in a human neuroblastoma cell line exposed to cysteamine-QDs and QDs modified by an antioxidant, N-acetylcysteine. We report new mechanisms of cytotoxicity induced by these QDs, including the i) upregulation of the Fas receptor, ii) lipid peroxidation, and iii) impaired mitochondrial function. Understanding the mechanisms underlying QD-toxicity will provide alternative ways of nanoparticle manipulations to make them more suitable tools in nanomedicine, specifically nano-oncology.
To investigate mechanisms underlying cell death induced by cadmium telluride (CdTe) QDs, we modified the surface of cysteamine-capped CdTe QDs with an antioxidant, N-acetylcysteine (NAC, Figure Figure1b),1b), a drug which has been found previously to protect cells against oxidative stress and QD-induced cytotoxicity . Cysteamine-capped (''unmodified'') QDs (Figure (Figure1a)1a) have amino groups at the surface and are positively charged (+14.2 mV). Covalent binding of NAC to cysteamine on the QD surface (Figure (Figure1c)1c) yielded NAC-conjugated QDs with a decreased net surface charge, and charge-charge complexation of NAC and cysteamine yielded NAC-capped QDs with carboxylic groups on the surface and a net negative charge of -9.8 mV (Figure (Figure1d).1d). Spectrofluorometric measurements revealed marked differences in the fluorescence intensities and QD stability in different media (see Additional file 1). In phosphate buffered saline (PBS), cysteamine-QDs show a red-shift with time but no change in fluorescence intensity, whereas, NAC-conjugated QDs decreased in fluorescence with time. NAC-capped QDs were the most stable in PBS, with no spectral shift and no loss of fluorescence within 24 hours.
To examine the cytotoxicity of cysteamine-QDs and NAC-modified QDs, we assessed the viability of SH-SY5Y human neuroblastoma cells by fluorescence-activated cell scanning (FACS), and their mitochondrial metabolism using a MTT reduction assay. Our FACS data show that cells exposed to 5 μg/mL of cysteamine-QDs, NAC-conjugated or NAC-capped QDs yielded distinct populations of dead cells (Figure (Figure2a),2a), suggesting significant toxicity induced by these QDs. Significantly less viability was observed in cells treated with cysteamine-QDs (52.2 ± 0.7%, p < 0.05) when compared to untreated control cells in serum-free medium (75.9 ± 9.1%). It is noteworthy that trophic factor deprivation, due to serum withdrawal, contributes to cell death which explains the approximately 25% decrease in viability in the absence of QDs (i.e. untreated control). NAC treatment can rescue cells in this trophic factor withdrawal paradigm . QD-induced cytotoxicity is prevented with cell pretreatment with 2 mM NAC (85.5 ± 5.7%; p < 0.01; Figure Figure2b),2b), confirming and complementing results from our previous studies demonstrating the effectiveness of NAC against both trophic factor deprivation and additional QD-insult . These multiple insults to neuroblastoma cells lead to cell death both by apoptosis and necrosis. The latter is characterized by mitochondrial and lysosomal swelling and perinuclear localization of these organelles . NAC-capped and NAC-conjugated QDs are still cytotoxic (65.6 ± 5.0%, p < 0.05 and 59.1 ± 5.1%, p < 0.05 respectively) compared to control.
Results of the FACS analyses were corroborated by data from measuring cellular MTT reduction (Figure (Figure2c).2c). Mitochondrial metabolic activity was most significantly reduced in cells in the presence of cysteamine-QDs (50.1 ± 5.2%; p < 0.01). NAC-conjugated QDs also significantly reduced the cellular mitochondrial activity (62.3 ± 6.5%; p < 0.01) compared to control. Cells treated with NAC-capped QDs, on the other hand, suffered less cytotoxic damage and showed significantly higher mitochondrial metabolic activity (90.2 ± 2.2%; p < 0.01) compared to cells treated with cysteamine-QDs or NAC-conjugated QDs. Cells pretreated with NAC, prior to cysteamine-QD addition, show significantly higher activity (106.1 ± 11.8%; p < 0.01) when compared to QD-treated cells, again reinforcing the protective role of free NAC against QD-induced toxicity.
QD-induced cytotoxicity involves oxidative stress, specifically via the production of reactive oxygen species (ROS) [12,15]. One cell-damaging, downstream effect of ROS production is the upregulation of the cell surface Fas receptor. FACS analyses revealed significant upregulation of Fas expression on the surface of SH-SY5Y cells treated with cysteamine-QDs (net mean fluorescence intensity (MFI) is 64.3 ± 5.5, p < 0.05) and NAC-conjugated QDs (net MFI = 57.1 ± 3.7, p < 0.05) when compared to untreated control cells (net MFI = 43.9 ± 1.1; Figures Figures3a3a and and3b).3b). No upregulation of Fas was observed in cells treated with NAC-capped QDs (net MFI = 42.1 ± 3.7), and Fas upregulation was completely inhibited in cells pretreated with NAC in the presence of cysteamine-QDs (net MFI = 41.5 ± 0.4), suggesting that QD-induced Fas expression is likely due to QD-mediated oxidative stress.
In addition, free Cd2+ released from QDs and the extent of QD uptake can contribute to the cell damage and eventually cell death. We measured intracellular and extracellular Cd2+ concentrations in SH-SY5Y cell cultures treated with QDs. Results from this study and from our recently published study  show that Cd2+ concentrations contribute to, but cannot fully explain QD-induced cytotoxicity (31.1 ± 1.7% and 58.0 ± 2.1% cytotoxicity induced by Cd2+ and QDs respectively), suggesting that impairment of cellular functions by QDs is multifactorial.
The extent of QD uptake was assessed by FACS analyses. Cells treated with cysteamine-QDs, NAC-conjugated and NAC-capped QDs show marked differences in QD uptake. In particular, cysteamine-QD-treated cells show an evident shift in fluorescence intensity compared to the untreated control and to both NAC-conjugated and NAC-capped QD-treated cells (Figure (Figure3c).3c). Quantitative measurements of the mean fluorescence intensity show that cysteamine-QDs were indeed taken up most avidly (net MFI = 17.8 ± 0.1; Figure Figure3d).3d). On the other hand, NAC-conjugated QDs (net MFI = 7.3 ± 0.6; p < 0.001) and NAC-capped QDs (net MFI = 2.1 ± 1.2; p < 0.001) were internalized significantly less than cysteamine-QDs. The net MFI for cells pretreated with 2 mM NAC (5.6 ± 0.8; p < 0.001) was significantly lower than in the absence of NAC (net MFI = 17.8 ± 0.1), suggesting that NAC either reduced QD uptake or partly quenched QD fluorescence. The latter is unlikely as spectral data show that these NAC-modified QDs have comparable, and in some cases even higher, fluorescence intensities as the unmodified QDs (see Additional file 1). On the other hand, measurements of intracellular Cd2+ show reduced Cd2+ content in NAC pretreated cells, supporting the notion that less QDs were internalized by the cells and that extracellular Cd2+ effects were also diminished by NAC.
The subcellular distribution of internalized QDs has previously been reported to induce ROS production and organelle damage [12,14]. Here we identify two intracellular targets of this QD-induced ROS, namely membrane lipids and mitochondria. In response to oxidative stress, cell surface and organellar membrane lipids may undergo peroxidation . We assessed lipid peroxidation by spectrofluorometric measurements of the fluorescent BODIPY-C11 dye and by confocal microscopy (Figures 4a, b). When compared to untreated control cells (100.0 ± 6.3%), cells treated either with cysteamine-QDs (70.2 ± 2.0%, p < 0.01) or NAC-capped QDs (76.6 ± 6.5%, p < 0.05) showed significantly reduced red (non-oxidized) to green (oxidized) ratios. Cells treated with NAC-conjugated QDs or pretreated with free NAC, in the presence of cysteamine-QDs, did not show significant lipid peroxidation compared to the untreated control.
Double labeling using BODIPY-C11 dye and MitoTracker Deep Red 633 revealed lipid peroxidation of the mitochondrial membranes as shown by confocal microscopy (Figure (Figure4b).4b). Co-localized oxidized BODIPY-C11(green) and MitoTracker Deep Red 633 (red-purple) appear as punctate yellow signals, suggesting local membrane lipid peroxidation within the mitochondria in cells treated with QDs.
Membrane lipid peroxidation can produce damaging aldehydes, and at the mitochondrial level, this can impair mitochondrial functions . Confocal microscopy analyses of cells stained with JC-1 clearly show that QD-treated cells have significantly reduced mitochondrial membrane potential (Δψm) (Figure (Figure4c).4c). Compared to the strong red fluorescence of JC-1 aggregates observed in the untreated control, QD-treated cells show an increased intensity in green fluorescence (JC-1 monomers) which correlates with a decrease in Δψm.
Initial reports on the potential toxicity of some types of quantum dots (QDs) [13,14,29] prompted the development of differently modified QDs as tools in the biological sciences. Several studies describing modifications to improve QD biocompatibility for their broad applications in the medical sciences were recently reported [10,30,31]. At the other end of the spectrum, research groups are also attempting to harness and apply QD toxicity in toxicotherapy. For instance, one study proposed the application of dopamine-conjugated QDs as inducers of cellular phototoxicity , while others are using QDs in photodynamic therapy  and to target different stages of cancers [11,34]. Using NAC-conjugated, NAC-capped and cysteamine-capped CdTe QDs, this study shows several cellular responses of human neuroblastoma cells to these nanoparticles. Surface-modified nanoparticles with NAC led to reduced cell death, decreased Fas expression and decreased mitochondrial membrane lipid peroxidation. The negatively charged NAC-capped QDs were the most benign, followed by NAC-conjugated QDs. Cysteamine-QDs, with a net positive surface charge, showed significant cellular uptake, as well as increased upregulation of Fas receptors on the cell surface and membrane lipid peroxidation, contributing to the impairment of mitochondrial and overall cell functions. In addition to surface charge, cytotoxicity is also affected by other physicochemical properties, including particle size, core-shell composition and capping [14,35,36].
QD biocompatibility can be easily altered by surface modifications, such as conjugation and capping with biomolecules and polymers [31,37,38]. The Hoshino group characterized the physicochemical properties of different surface-modified CdSe QDs and reported that these surface modifications affect QD surface potential, QD fluorescence and QD-induced cytotoxicity . In our study, we found that QD surface conjugation and capping with an antioxidant, N-acetylcysteine (NAC), reduced QD uptake and cytotoxicity (Figures (Figures22 and and3).3). Moreover, pretreatment of cells with free NAC fully protected cells from QD-induced cytotoxicity (Figure (Figure2b),2b), as demonstrated in our previous study in a different cell line . NAC can protect cells both from apoptosis and necrosis. Mechanisms of the cytoprotective action of NAC are well-documented, and involve NAC acting (i) as a direct thiol antioxidant, (ii) as a glutathione precursor, (iii) as a transcription regulator for genes involved in cellular homeostasis, and (iv) as a cell survival promoter via inhibition of apoptotic pathways including JNK and p38 .
Highly metabolically active mitochondria are particularly sensitive and vulnerable targets to cellular stress . Cells treated with QDs undergo a change in mitochondrial membrane potential (Δψm) (Figure (Figure4c).4c). Membrane depolarization has been widely associated with the release of the apoptotic factor, cytochrome c, which amplifies pro-apoptotic caspase cascades, promoting cell death [12,25]. Among the regulators of mitochondrial membrane potential, cardiolipin, a mitochondrial membrane specific lipoprotein, is of particular relevance in neuronal cells [39,40]. The abundance of cardiolipin in the membranes of the mitochondria maintains the membrane potential and regulates the release of cytochrome c. Upon cellular stress, cardiolipin, along with other membrane lipids, is degraded due to lipid peroxidation, and the membrane potential is no longer stable, resulting in an uncontrolled release of mitochondrial content [40,41]. In addition to causing membrane instability and increasing the vulnerability of the cell to subsequent insults , lipid peroxidation can also generate harmful and relatively stable aldehyde products which add to the oxidative stress. One of these damaging aldehydes is 4-oxo-2-nonenal (ONE), which acts by activation of the p53 signaling pathway and induces apoptosis in SH-SY5Y neuroblastoma cells .
Besides intracellular targeting at the mitochondrial level, QD treatment leads to an upregulation of cell surface Fas expression (Figures (Figures3a3a and and3b).3b). The Fas receptor, when activated by Fas ligand, associates with FADD which recruits caspase-8 or caspase-10, and forms the death-inducing signaling complex (DISC). Caspases-8/10 autocatalyze their own cleavage [43-45], triggering a cascade of caspase activation that culminates in apoptosis. This cascade may be further amplified by cleavage of the caspase-8/10 substrate Bid, which then inserts into the mitochondrial membrane, resulting in loss of Δψm and release of cytochrome c, further accelerating apoptosis. Fas has been implicated as an inducer of apoptosis under conditions of high in vivo oxidative stress [46-48], and recent studies show that Fas expression may also be triggered upon activation of proapoptotic transcription factors, such as FOXO3 .
Nanoparticles, such as the CdTe QDs investigated here, enter cells and can get sequestered within different organelles, changing organellar morphologies and obstructing their functions, leading eventually to cell death of different types [17,50,51]. For instance, our recent study in human breast cancer cells  showed that QDs induce enlargements of lysosomes and mitochondria, both of which are morphological indications of necrotic cell death. On the other hand, intracellular accumulation of unprotected or unstable QDs can eventually result in QD degradation and Cd2+ release from the QD core, initiating apoptosis. The extent of apoptosis in neuroblastoma cells and Cd2+ released are, however, not strongly correlated, suggesting additional contributors to cell death aside from the free Cd2+.
Neuroblastoma cells that were deprived of serum-derived trophic factors are more susceptible to additional insults induced by QDs (i.e. ROS, Cd2+), leading to both type I (apoptosis) and type III (necrosis) cell death . Under the circumstances in which QDs could be employed for the detection and elimination of neuroblastoma, one should bear in mind not only the physical properties of QDs but also the vulnerability of healthy tissues surrounding the tumour, the rate of QD sequestration and the rate of metal elimination from the body . Collectively, earlier and current findings suggest that cell pre-conditioning, combined with modifications of the QD surface with NAC and a tumour-specific ligand (e.g. Trk mimetics to target Trk receptors) could yield an improved nano-oncological therapeutic, sensitizing or diagnostic agent for neuroblastomas.
Results from this study provide new mechanistic data (summarized in Figure Figure5)5) on the much debated issue of QD toxicity. Cadmium telluride (CdTe) QD-induced cytotoxicity depends on multiple QD properties including QD core size, stability in biological media and surface chemistry which determine the extent of cellular internalization. Mechanisms of CdTe QD-induced toxicity include multiple organelle damage and involve increased Fas receptor expression and cell membrane lipid peroxidation in SH-SY5Y neuroblastoma cells. These damages bring about cell death both by apoptosis and necrosis. Understanding the mechanisms underlying QD toxicity is important as QDs and other nanoparticles are promising tools in the field of nano-oncology as potential imaging agents, photosensitizers, biosensors and nanotherapeutics.
Tellurium powder (200 mesh, 99.8%), sodium borohydride (99%), cadmium perchlorate hydrate, N-acetylcysteine (99%) and cysteamine hydrochloride (98%) were purchased from Sigma-Aldrich. Milli-Q water (Millipore) was used as a solvent. Photoluminescence measurements were carried out at room temperature using a Cary Eclipse Fluorescence spectrometer. The excitation wavelength was set at 400 nm. The excitation and emission slits were set at 5 nm. Dialysis was performed using spectra/por molecularporous membrane tubing (Spectrum Laboratories, Inc.) with a 6000–8000 Da molecular weight cutoff. Centrifugation was performed with Eppendorf centrifuge 5403 (10,000 rpm) and Eppendorf centrifuge 5415 C (14,000 rpm).
Sodium borohydride (0.8 g, 21.1 mmol) was dissolved in water (20 mL) at 0°C under N2 atmosphere. Tellurium powder (1.28 g, 10 mmol) was added portionwise and the mixture was stirred at 0°C for 8 h under N2 atmosphere. The reaction mixture was stored at 4°C in the dark and used in the next step.
The thiol capped-QDs were prepared as described . Briefly, cadmium perchlorate hydrate (500 μL, 1 M aqueous solution) and cysteamine hydrochloride (300 mg, 2.64 mmol) were dissolved in 200 mL of N2 saturated Milli-Q water. The pH of the solution was adjusted to 5.1 with 1N NaOH aqueous solution prior to addition of an aliquot of the previously prepared NaHTe solution (200 μL). The reaction mixture was heated to reflux for 25 min under N2. The resulting QD solution was dialyzed against Milli-Q water for 4 h then concentrated to 15 mL using a rotary evaporator. QDs were precipitated using MeOH/CHCl3 (1:1, v/v) then collected by centrifugation. The QDs were washed with MeOH/CHCl3 (1:1, v/v) two times then dried under vacuum. The QDs were used as solutions either in deionized water or in PBS buffer.
Cadmium perchlorate hydrate (500 μL, 1 M aqueous solution) and N-acetylcysteine (400 mg, 2.45 mmol) were dissolved in 200 mL of N2 saturated Milli-Q water. The pH of the solution was adjusted to 10.5 with 1N NaOH aqueous solution prior to addition of an aliquot of the previously prepared NaHTe solution (200 μL). The reaction mixture was heated to reflux for 25 min under N2. The resulting QD solution was dialyzed against Milli-Q water for 4 h then processed as above.
Solutions of NAC (4 mM) were freshly prepared in water mixed with cysteamine capped (+) CdTe QD in water (2 mg/mL, λem = 542 nm) followed by 1-ethyl-3-(3'-dimethylaminopropyl)carbodiimide (EDC; 12 mg, 77.3 μmol) addition. The reaction mixture was incubated for 3 h at room temperature with occasional shaking. The mixture was purified by dialysis against water for 4 h. The emission wavelength of the resulting solution was 533 nm. The NAC-conjugated QDs were used as a solution in water. Zeta potentials of all QD preparations were measured using Zetasizer Nano ZS (Malvern Instruments, Worchestershire, UK).
The human neuroblastoma cell line SH-SY5Y was obtained from ATCC and cultured (37°C, 5% CO2) in DMEM medium containing phenol red and 10% FBS (Gibco, Burlington, ON, Canada). Cells were used at 2–8 passages. For spectrofluorometric and colorimetric assays, cells were cultured in 24-well plates (Sarstedt, Montreal, QC, Canada) at a density of 105 cells/cm2.
One hour prior to treatments, medium containing serum was aspirated, and cells washed with serum free medium. Fresh serum free medium was added to all wells, including the untreated control (Ctrl). An additional set of control cells, grown in 10% FBS, was used to account for changes in cell morphology, cell number and metabolic activity due to the serum withdrawal.
Cells were treated with QDs (5 μg/mL) for different time periods as specified in individual figure legends. QD solutions (5 μg/mL) were prepared from the stock (2 mg/mL) by dilution in serum free cell culture medium. Cells were incubated with QDs for a maximum of 24 h before biochemical analysis or live cell imaging.
NAC was dissolved in PBS (400 mM), and was added to the culture medium 2 h before QDs. All treatments were done in triplicates or quadruplicates in three or more independent experiments.
SH-SY5Y cells were treated with 5 μg/ml QDs (NAC-modified and unmodified) and/or 2 mM NAC (as indicated) for 24 h at 37°C/5% CO2 in media supplemented with 10% FBS. Adherent and non-adherent cells were harvested and pooled so as not to lose apoptotic cells which may have detached from the plastic substrate. Cells were resuspended at 1 × 106 cells/ml in FACS buffer (PBS + 1 % FCS). Fas expression was determined by labeling cells with phycoerythrin (PE) conjugated anti-human Fas/CD95 (clone DX2, BD Biosciences), and PE conjugated isotype-matched control antibodies (mouse IgG1 kappa, BD Biosciences) for 30 min on ice. Cells were washed twice and resuspended in 300 μl FACS buffer. Samples analysed for viability and/or for quantum dot-associated fluorescence alone (FL1, PMT 488–540 nm) were not labeled with antibodies. 10,000 events per sample were acquired on a Becton Dickinson FACScan flow cytometer. Data were analyzed using CellQuest software. Fas expression was determined as follows: Net Fas expression = Fas mean fluorescence intensity (MFI) – isotype control MFI for each individual sample, then averages and standard deviations of three independent replicates were calculated.
Colorimetric MTT (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl tetrazolium bromide, Sigma) assays were performed to assess the mitochondrial activity of cells treated as described above. After 24 h treatment, media was removed and replaced with drug-free, serum-free media (500 μL/well). 50 μL of stock MTT (5 mg/mL) was added to each well and cells were then incubated for one hour at 37°C. Media were removed, cells were lysed and formazan dissolved with DMSO. Absorbance was measured at 595 nm using a Benchmark microplate reader (Bio-Rad, Mississauga, ON, Canada). All measurements were done in triplicates in three or more independent experiments.
Cells were treated with the fluorescent dye BODIPY 581/591 C11 (BODIPY-C11, Molecular Probes), which inserts into lipid membranes and allows for quantitative assessment of oxidized versus non-oxidized lipids by fluorescing green or red, respectively. Cells were stained for 30 min with a 10 μM solution of BODIPY-C11 prior to QD treatment. After the QD treatment, lipids were extracted from the cells according to the Folch method  by incubating twice with a mixture of chloroform and methanol (2:1 (v/v)). After extraction, 0.2 volumes of 0.9% NaCl solution were added and the chloroform-containing phase was collected. After evaporating the chloroform and dissolving the lipids in isopropanol, spectrofluorometric readings were taken using the SpectraMax Gemini XS microplate spectrofluorometer (Molecular Devices Corporation, USA). Data were analyzed using the SOFTmax Pro 4.0 program. All values are presented as normalized means ± SEM relative to the respective serum-free control (taken as 100%).
Images were acquired with a Zeiss LSM 510 NLO inverted microscope. Cells were grown in 8-well chamber slides (Lab-Tek, Nalge Nunc International, Rochester, NY, USA). QDs were added to designated wells and the cells were incubated for the times indicated. Mitochondria were stained with MitoTracker Deep Red 633 (1 μM, 1 min, Molecular Probes; λex 644 nm, λem 665 nm) and imaged using HeNe 633 nm excitation laser and LP 650 filter. Lipid peroxidation was visualized using BODIPY-C11 (Molecular Probes; non-oxidized: λex 581 nm, λem 595 nm; oxidized: λex 485 nm, λem 520 nm) with the Argon 488 nm excitation laser and LP 520 nm filter, and the HeNe 543 nm laser and LP 560 filter. Mitochondrial depolarization was determined using JC-1 (15 μM, 30 min, Molecular Probes; monomer: λex 485 nm, λem 530 nm; aggregate: λex 535 nm, λem 590 nm). The potential-sensitive color shift was monitored using the same set of lasers and filters as BODIPY-C11. Before imaging, cells were washed with PBS or with serum-free medium. No background fluorescence of cells was detected under the settings used. Images were acquired at a resolution of 512 × 512 and 1024 × 1024. Quadruplicate samples were analyzed in all the imaging experiments. Scan size was 146.2 μm × 146.2 μm. Figures were created using Adobe Photoshop.
Data were analyzed using SYSTAT 10 (SPSS, Chicago, IL, USA). Statistical significance was determined by Student's t-tests with Bonferroni correction. Differences were considered significant where *p < 0.05, **p < 0.01, ***p < 0.001.
CdTe, cadmium telluride; NAC, N-acetylcysteine; QD, quantum dot; ROS, reactive oxygen species; FACS, fluorescence-activated cell sorting; MTT, 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide; BODIPY-C11, 4,4-difluoro-5-(4-phenyl-1,3-butadienyl)-4-bora-3a,4a-diaza-s-indacene-3-undecanoic acid; JC-1, 5,5',6,6'-tetrachloro-1,1',3,3'-tetraethylbenzimidazolylcarbocyanine iodide;
The author(s) declare that they have no competing interests.
DM initiated and guided these studies. DM drafted and AOC finalized the manuscript. AOC, SJC, JD and JL carried out the experiments. All authors read and approved the final manuscript.
PL spectra (stability) of CdTe nanoparticles in water and PBS.
This work was supported by the Juvenile Diabetes Research Foundation (Canada) and the Canadian Institutes of Health Research. The authors would like to thank J. Laliberté for assistance with confocal microscopy and U. Koppe with lipid peroxidation experiments.