Amylase-Protected Ag Nanodots for in vivo Fluorescence Imaging and Photodynamic Therapy of Tumors
Authors Wen S, Wang W, Liu R, He P
Received 2 October 2019
Accepted for publication 21 February 2020
Published 14 May 2020 Volume 2020:15 Pages 3405—3414
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 2
Editor who approved publication: Dr Linlin Sun
Shuguang Wen,1– 3,* Weili Wang,4,* Ruimin Liu,3 Pengcheng He1
1Department of Hematology, The First Affiliated Hospital of Xi’an Jiaotong University, Xi’an 710061, People’s Republic of China; 2Department of Hematology, The First Affiliated Hospital of Zhengzhou University, Zhengzhou 450052, People’s Republic of China; 3Basic Medical College, Henan University, Kaifeng 475000, People’s Republic of China; 4State Key Laboratory of Radiation Medicine and Protection, School for Radiological and Interdisciplinary Sciences (RAD-X), Collaborative Innovation Center of Radiological Medicine of Jiangsu Higher Education Institutions, Soochow University, Suzhou 215123, People’s Republic of China
*These authors contributed equally to this work
Correspondence: Pengcheng He
Department of Hematology, The First Affiliated Hospital of Xi’an Jiaotong University, No. 277 Yanta West Road, Xi’an 710061, People’s Republic of China
Tel +86 189 9123 2609
Email [email protected]
Background: Fluorescent metallic nanodots (NDs) have become a promising nanoprobe for a wide range of biomedical applications. Because Ag NDs have a high tendency to be oxidized, their synthesis and storage are a big challenge. Thus, the method for preparing stable Ag NDs is urgently needed. Surface modification and functionalization can enrich the capability of Ag NDs.
Methods: In this work, fluorescent Ag NDs were synthesized in deoxygenated water by using porcine pancreatic α-amylase (PPA) as the stabilizing/capping agent. The absorption and fluorescence of PPA-protected Ag NDs ([email protected]) were measured with a spectrophotometer and a spectrofluorometer, respectively. The morphology of [email protected] was characterized by high-angle annular dark-field (HAADF) scanning transmission electron microscopy (STEM). The biocompatibility of [email protected] was evaluated by tetrazolium (MTT)-based assay. PolyLys-Cys-SH (sequence: KKKKKKC) peptides were conjugated to [email protected] via heterobifunctional crosslinkers. PolyLys-Cys-linked [email protected] absorbed 5-aminolevulinic acid (ALA) by electrostatic interaction at physiological pH. The capability of tumor targeting was evaluated by intravenously injecting [email protected] into 4T1 breast cancer xenograft mouse models. Photodynamic therapy (PDT) against tumors was performed under 635 nm laser irradiation.
Results: [email protected] emitted at 640 nm with quantum yield of 2.1%. The Ag NDs exhibited strong photostability over a long period and a fluorescence lifetime of 5.1 ns. [email protected] easily entered the cells to stain the nuclei, showing the capabilities of living cell imaging with negligible cytotoxicity. ALA-loaded [email protected] ([email protected]) presented the superiority of passive tumor targeting via the enhanced permeability and retention (EPR) effect. Tumors were visualized in the near-infrared (NIR) region with reduced background noise. ALA molecules released from [email protected] was converted into the photosensitizer (PS) of protoporphyrin IX (PpIX) intracellularly and intratumorally, which greatly improved the PDT efficacy.
Conclusion: Our approach opens a new way to design a novel theranostic nanoplatform of [email protected] for effective tumor targeting and fluorescence image-guided PDT.
Keywords: α-amylase, Ag nanodots, peptides, targeted imaging, photodynamic therapy
Noble metal (Au, Ag, Cu and Pt) nanodots (NDs) have recently become a useful tool in diverse biomedical applications.1–11 These NDs exhibit discrete electronic structure, photoluminescence (PL), intrinsic chirality, catalytic activity, and paramagnetism.12–18 Moreover, the toxicity of NDs is much lower than heavy metal-containing fluorescent nanoprobes like quantum dots, making them as a promising alternative for biological imaging.2,4,8–11 So far, Ag NDs have not attracted as much attention as Au NDs due to their rapid decomposition to Ag ions upon exposure to water and oxygen, which is a big issue remaining unsolved.19 Unfortunately, the synthetic strategies of Au NDs are not all working for Ag NDs. For example, a few proteins such as bovine serum albumin (BSA), lysozyme, apo-α-lactalbumin, horseradish peroxidase (HRP) and bovine pancreatic ribonuclease A (RNase A) were reported to synthesize Au NDs.20–24 The redox-active Tyr and Trp residues of proteins are too weak to reduce Ag,20 since the redox potential of Ag+/Ag is as low as ~0.80 V. Hence, a stronger reducing agent like NaBH4 is needed. Xie and coworkers were the first group to report the synthesis of Au NDs stabilized by BSA.20 Shortly afterwards, the method was extended by Guével et al to prepare Ag NDs based on the reduction by NaBH4.25 However, the strong reducibility of NaBH4 made the reaction difficult to be controlled. Moreover, the protein coating increased the overall size. Likewise, Yu et al reported that fluorescent Ag NDs were synthesized within cellular nucleoli by photoactivation, depending on the high affinity of nucleolin to Ag ions.26
In this paper, we employ porcine pancreatic α-amylase (PPA) as the stabilizing agent to synthesize fluorescent Ag NDs. As a single polypeptide chain, PPA (molecule weight: 51–54 kDa) is comprised of 475 residues to hydrolyze α-bonds of α-linked polysaccharides.27 It has two thiol groups and four disulfide bridges to offer a strong affinity for Ag. PPA-protected Ag NDs ([email protected]) exhibit strong red emission with peak maximum at ~640 nm and robust photostability, benefiting from our established method that can prevent Ag from tarnishing. The condense PPA coating isolates the Ag surface from corrosive O2 in water for high stability. Moreover, Ag NDs can be internalized by living cells and even enter the nuclei to show the capability of cell imaging with negligible cytotoxicity. To construct a multifunctional nanoplatform, positively charged lysine-rich polyLys-Cys-SH (sequence: KKKKKKC) peptides are covalently conjugated to Ag NDs by PEGylated SMCC crosslinker, and then negatively charged 5-aminolevulinic acid (ALA) is electrostatically adsorbed at physiological pH to form ALA-loaded [email protected] ([email protected]). Unlike many emerging therapeutic nanoplatforms,28–30 ALA has been clinically used as a prodrug to induce the tumor accumulation of protoporphyrin IX (PpIX) for photodynamic therapy (PDT).31–33 [email protected] can passively target tumors through the enhanced permeability and retention (EPR) effect, and be endowed with fluorescent image-guided enhanced PDT of tumors.
Porcine pancreatic α-amylase (PPA), 5-aminolevulinic acid (ALA), Rhodamine 6G (R6G), acetylacetone, formaldehyde and Dulbecco’s Modified Eagle Medium (DMEM) were purchased from Sigma-Aldrich. SM (PEG)12 crosslinkers and Slide-A-Lyzer™ Dialysis Cassettes (MWCO: 10 KDa) were purchased from Thermo Fisher Scientific Co., Ltd. Silver nitrate (AgNO3), sodium hydroxide (NaOH), sodium borohydride (NaBH4) and dimethyl sulfoxide (DMSO) were purchased from Sinopharm Chemical Reagent Co., Ltd. All chemicals were used as received without further purification. All solutions were prepared using purified water with resistivity of 18 mΩ cm−1 as the solvent. The water was deoxygenated before use with a nitrogen purge for 1 h at the flow rate of 25 mL/s.
Synthesis of [email protected]
In a typical synthesis, 1 mL of AgNO3 solution (10 mM) was mixed with 1 mL of PPA solution (50 mg/mL) under stirring in an ice bath for 1 min. Thereafter, 0.1 mL of NaOH (1 M) was dropwise added into the mixture. 0.05 mL of NaBH4 solution (2 mM) was added. The color of solution changed from colorless to light brown and then to reddish brown, which indicated the formation of Ag NDs. The resultant solution was dialyzed with a dialysis cassette (MWCO: 10 KDa) in PBS solution (pH 7.4) and kept at 4°C in darkness for the follow-up use.
Conjugation of PolyLys-Cys-SH (KKKKKKC) to [email protected]
Two milligrams of polyLys-Cys-SH peptides were dissolved in 20 μL of DMSO and mixed with 25 mg/mL [email protected] in 1 mL of PBS solution (pH 7.2). Then, SM (PEG)12 crosslinkers with 1 mM final concentration were added and stirred for 2 h at 4°C. The NHS esters of SM (PEG)12 reacted with the primary amines of PPA to form amide bonds, while the maleimides of SM (PEG)12 reacted with the sulfhydryl groups of polyLys-Cys-SH peptides to form thioether bonds. Thus, polyLys-Cys-SH peptides were covalently conjugated to [email protected] The resultant solution was dialyzed for 1 h with a dialysis cassette in PBS solution (pH 7.4). Peptide-linked [email protected] was purified and kept at 4°C in darkness.
Electrostatic Adsorption of 5-Aminolevulinic Acid (ALA)
Conjugation of ALA to [email protected] modified with polyLys-Cys-SH peptides was achieved by electrostatic interaction between ALA and the positively charged lysine residues. Four milligrams of ALA was dissolved in 2 mL of Dulbecco’s Modified Eagle Medium (DMEM) and sterilized with filtration through a 0.2 μm filter. PolyLys-Cys-linked [email protected] were also sterilized. After that, 1 mL of ALA solution was mixed with 200 µL of polyLys-Cys-linked [email protected], and the system pH was adjusted to pH 7.4 with 1 N NaOH solution. The resultant solution was dialyzed for 1 h with a dialysis cassette (MWCO: 10 KDa) in PBS solution (pH 7.4) to remove unbound ALA. After the synthesis of [email protected], the unbound ALA was collected and its concentration in solvent was determined using a method reported by AI-Kassas et al.34
ALA loading was calculated from:
Fluorescence spectra were measured with a Hitachi F-4600 fluorometer. UV-visible absorption spectra were recorded with a Shimadzu UV-2600 spectrophotometer. Ambient-light and dark-field photographs of [email protected] were captured with an Olympus Stylus 7010 digital camera. Time-resolved fluorescence measurement was carried out with an FLS 920 fluorescence lifetime and steady-state spectroscopy. Scanning transmission electron microscopy (STEM) was recorded using a TEM/STEM microscope with an FEI Tecnai G2 F20 field emission gun and fitted with a Fischione HAADF detector, an 80 mm2 Oxford Instruments X-Max silicon drift detector (SDD) and a Gatan Orius. TEM sample was prepared by drop-casting [email protected] on copper grids coated with ultrathin carbon film and dried at ambient temperature and pressure conditions. Dynamic light scattering (DLS) and zeta potential (ZP) were carried out with a Mastersizer 3000 laser diffraction particle size analyzer.
Calculation of Quantum Yield
The quantum yield (Φ) of [email protected] is determined by the relative method and calculated according to the following equation:
where ΦR is the quantum yield of the reference R6G (ΦR=94%); I and IR are the integrated fluorescence intensities for [email protected] and R6G, respectively; A and AR are the absorbance values of [email protected] and R6G, respectively.
Cell Viability Assay
Mouse breast (4T1) cancer cells were cultured as adherent monolayers in plastic tissue culture dishes in RPMI-1640 medium (ATCC, USA) supplemented with 10% heat-inactivated Fetal Bovine Serum (ATCC, USA) and antibiotic solution (1 mL per 100 mL of cell culture medium, Thermo Fisher Scientific, USA). The cells were cultured in 75 cm2 culture flasks and maintained within a Thermo Scientific Forma Direct-Heat CO2 incubator (37°C, 5% v/v CO2 atmosphere and 95% relative humidity). The cytotoxicity of [email protected] on 4T1 cells was assessed by MTT (3(4,5-dimethylthiazol-2-yl) 2,5-diphenyltetrazolium bromide) assay. Cells were seeded into a 96-well plate at the density of 1.0×104 cells/well in 100 μL of complete growth medium. After overnight initial plating, the medium was exchanged for fresh medium supplemented with [email protected] within a range from 0, 10, 100 to 200 µg/mL for 48 h with three wells per condition. [email protected] were dissolved in 1×PBS, and the final concentration was obtained by diluting [email protected] with complete culture medium. Fresh medium was used as untreated control group. Twenty microliters of MTT working solution (5 mg/mL) was added. After 4 hof incubation at 37°C, culture supernatant was removed from the wells, and the formazan crystals were dissolved in 150 µL of DMSO. One hundred microliters of the supernatant was transferred into a new 96-well plate after centrifugation (1000 g, 5 min). The samples were analyzed with an EL×800 absorbance microplate reader (BioTek Instruments, Winooski, USA) by measuring 570 nm reading with background correction at 630 nm. Healthy cells were used as control, so that the cell viability is regarded as 100%. The cell viability of [email protected] cells was indicated as the percentage (%) of the control.
4T1 cells were plated in a 24-well plate (1×105 cells/well) and incubated with gradient concentrations (0, 10, 100, and 200 µg/mL) of [email protected] for 48 h at 37°C. The cells were gathered and washed twice with PBS, and resuspended in 200 µL of binding buffer and incubated with 5 µL of annexin V-FITC and 1 µL of PI at room temperature, hatched at room temperature (RT) for 20 min in the dark. Then, 400 μL of binding buffer was added, gently mixed, put over the ice and immediately analyzed using a fluorescence-activated cell sorting (FACS) system (FC500 flow cytometer).
Tumor-Targeted Imaging in vitro and in vivo
In vitro cell imaging: Cell culture medium was changed daily. The cell medium was replaced by the fresh on the day of the test. After 2 h of incubation with [email protected], the cells were washed thrice with 1×PBS buffer to wipe out unbound [email protected] [email protected] cells were under microscopic observation with a Leica SP5 confocal microscope.
In vivo tumor-targeted imaging: 100 µL of [email protected] was intravenously (IV) injected into 4T1 tumor xenografted nude mice models (n=3). The time-course in vivo and ex vivo imaging was carried out with an IVIS® Spectrum in vivo imaging system.
PDT in vitro and in vivo
In vitro PDT: 4T1 cells (1×104 cells/100 µL) were seeded in 96-well plates and placed in the incubator at 37°C for 24 h. The medium was then replaced with fresh one containing 100 µM [email protected] or [email protected] After 6 h, the medium was replaced again with 1×PBS. Cells were illuminated under a 635-nm laser at the fluence rate of 100 mW/cm2 for 10 min. Immediately afterwards, PBS was replaced again with fresh medium. However, the control group was not exposed to ALA or laser irradiation. After 24 h, cell viability was tested using MTT assay. The absorbance of samples was measured with the EL×800 microplate reader by measuring 570 nm reading with background correction at 630 nm.
In vivo PDT: 12 nude mice bearing 4T1 tumors were randomly distributed into four groups: (1) control group, injection of PBS (100 μL); (2) “laser” group, 635nm-laser irradiation (0.5 W/cm2, 10 min); (3) “[email protected]” group, injection of [email protected] (100 μL, 100 µg/mL); (4) “[email protected] + laser” group, injection of [email protected] (100 μL, 100 µg/mL) with 635 nm laser irradiation (0.5 W/cm2, 10 min). For group (4), PDT was carried out on the tumor site at 4 h post-injection. Tumor volume and body weight were recorded every 4 days over a 24-day period. After the treatment, major organs (heart, liver, spleen, lung and kidney) and tumors of mice were collected for the hematoxylin and eosin (H&E) stain.
Results and Discussion
Synthesis of [email protected]
Figure 1 describes the synthesis procedures of fluorescent Ag NDs based on the kinetic template effect of PPA. Firstly, AgNO3 was mixed with PPA in aqueous solution under vigorous stirring, and the metal cations were coordinated to cysteine (Cys) residues. Secondly, NaBH4 was added to reduce the Ag ions from +1 to 0. Four disulfide bonds (S-S) broke into eight thiols to stabilize the Ag NDs with two extra thiols. NaBH4 played a vital role in the synthesis of Ag NDs, because too much NaBH4 resulted in large, non-fluorescent Ag NPs. Thus, the synthesis has to be progressed in low temperature to decelerate the redox reaction. As the solvent, water was deoxygenated beforehand with a nitrogen purge for 1 h at the flow rate of 25 mL/s to minimize dissolved oxygen, so [email protected] were less likely to be oxidized throughout manipulation. [email protected] were purified by dialysis in 1×PBS and stored at 4°C in darkness for subsequent use.
Figure 1 Schematic of synthesis of fluorescent [email protected]
Photophysical Properties of [email protected]
As shown in Figure 2A, the UV/vis absorption of [email protected] has a small shoulder peak at ~420 nm because of surface plasma resonance (SPR) absorption. Figure 2B presents that nearly a half of the band falls in the red spectrum (580 to 700 nm) with a peak maximum at 643 nm and a narrow full width at half maximum (FWHM) of ~126 nm. The quantum yield (QY) of [email protected] was determined as 2.1% using Rhodamine 6G (R6G) in ethanol as the reference standard (QY = 94%). As shown in Figure 2C, the strong photostability is noted that the fluorescence intensity of [email protected] deceased slowly (<10%) over a 30-day storage, confirming that the oxidation process was inhibited to a great extent. Although O2 gas had been largely removed from water by N2 gas bubbling, the air could still dissolve in water over time. However, the re-dissolved O2 had little effect on the fluorescence intensity of [email protected], indicating that PPA might form a condense protein coating to isolate the Ag NDs from the environment. Changes in pH also had unobvious effect on the intensity (Figure 2D). All the advantages of [email protected] are favorable for in vivo fluorescence imaging. As shown in Figure S1, the time-resolved fluorescence decay curve is well fitted using a three-exponential decay function with an average lifetime (T) of 5.12 ns (T1 = 4.69 ns, 45.47%; T2 = 1.21 ns, 7.48%; T3 = 12.68 ns, 47.05%).
Figure 2 (A) Typical UV–vis absorption and (B) normalized fluorescence spectra of [email protected] in aqueous solution. (C) Effect of air oxidation on fluorescence intensity of [email protected] over a long storage (30 days). (D) Effect of pH on fluorescence intensity of [email protected] (λex: 490 nm).
Morphology and Size Analysis of [email protected]
High-angle annular dark-field (HAADF) scanning transmission electron microscopy (STEM) is advantageous for morphological analysis of metallic NDs. The image contrast of Ag NDs is proportional to the atomic number (Z) squared of Ag element. As shown in Figure 3A, the white dots represent the Ag NDs, and the average diameter is 1.72 ± 0.29 nm (Figure 3 inset). The dynamic light scattering (DLS) spectrum of Figure 3B presents that the hydrodynamic diameter of [email protected] is determined to be 6–7 nm, indicating that the protein contributed little to size increase. As shown in Figure 3C, the matrix-assisted laser desorption/ionization-time of flight (MALDI-TOF) mass spectrometry (MS) spectrum confirms that [email protected] have multiple species of different molecular weights, but the majority of them are composed of 19 Ag atoms. It is worth mentioning that the Ag NDs were likely detached from the PPA coating during the MS measurement probably due to the bond breaking by the laser.
Figure 3 (A) HAADF-STEM image and particle size analysis. (B) DLS spectrum. (C) MALDI-TOF MS spectrum of [email protected]
Cell Imaging with [email protected] and PDT with [email protected]
The ultrasmall size, good photostability and bright emission of [email protected] are favorable for sensitive cell imaging. As shown in the confocal laser scanning microscopy (CLSM) images of Figure 4A, 4T1 cells exhibit bright red emission after 2 h of incubation with [email protected] The nuclei gave red fluorescent signals overlapping with the signal of 4′,6-diamidino-2-phenylindole (DAPI) that stains the nuclei only. The result indicates that [email protected] passed through lysosomal and endosomal membrane to enter the nuclei without nuclei-targeting agents. Unlikely, many other NPs tend to end up in lysosomes and endosomes after cellular uptake. Thus, further investigations are needed to explain this behavior. Flow cytometric assay was used for viability assessment of the cells treated with various concentrations (0, 10, 100 and 200 µg/mL) of [email protected] As shown in Figure 4B, more than 90% of the cells are alive while apoptotic cells were less than 5% as exposing to 10 or 100 µg/mL [email protected] Although the FACS data confirm that the high concentration (such as 200 µg/mL) of [email protected] resulted in slightly cytotoxic effect (Figure 4C), they were biosafe over the abroad range of up to 100 µg/mL. To synthesize a theranostic nanoplatform, positively charged polyLys-Cys-SH (KKKKKKC) peptides were conjugated to the PPA coating via covalent coupling between amine (-NH2) and sulfhydryl (-SH) groups using a hetero-bifunctional crosslinker of SM(PEG)12 (Figure 5A). As the precursor of PpIX, negatively charged ALA was absorbed to the peptides by electrostatic adsorption to construct ALA-loaded [email protected] ([email protected]), the hydrodynamic diameter of which reached ~21 nm (Figure 5B). However, ALA can be released when the surrounding pH reduces to pH 5 such as endosomal or lysosomal interior (Figure 5C). As shown in Figure 5D, the large portion (~70%) of cells are killed under 635-nm laser irradiation with the power density of 100 mW/cm2 for 10 min in the presence of [email protected] However, the laser or [email protected] alone was incapable of killing the cells.
Figure 4 (A) Confocal laser scanning microscopy (CLSM) images of 4T1 breast cancer cells incubated with [email protected] for 2 h. Scale bar: 200 nm. (B) Flow cytometric analysis and (C) apoptosis percentage of 4T1 cells after incubating with 0, 10, 100 and 200 µg/mL of [email protected]
Figure 5 (A) Schematic of conjugation of polyLys-Cys-SH peptide to [email protected] at neutral pH; ALA loading to and releasing from [email protected] at acidic pH. (B) DLS spectrum of [email protected] (C) Cumulative amount of ALA released from [email protected] at pH 5.0 and pH 7.4. (D) Cell viability of different treatment groups (*p<0.05).
Tumor-Targeted Imaging and PDT with [email protected]
As depicted in Figure 2B, a large portion of emission spectrum of [email protected] falls in the NIR region (λ>700 nm), which suggests that they are suitable for fluorescence imaging to promote the signal-to-noise ratio (SNR). Indeed, the mouse shows fairly low autofluorescence background at pre-injection (Figure 6A). For in vivo fluorescence imaging, 200 µL of [email protected] (100 µg/mL) was intravenously injected into a mouse bearing 4T1 tumor xenograft. Figure 6A shows that [email protected] starts to accumulate in the tumor area as quickly as 0.5 h post-injection (p.i.), where fluorescent signals gradually become strong. The tumor area exhibited the highest SNR value at 2 h p.i., but afterwards the intensity became weaker. The results definitely indicate that [email protected] was capable of passive tumor targeting via the enhanced permeability and retention (EPR) effect. At 10 h p.i., the mouse was sacrificed to collect its major organs including heart, spleen, liver, kidney, lung and tumor for ex vivo imaging (Figure 6B). As observed, the tumor gives very strong signals, while a large number of [email protected] retained in the reticuloendothelial system (RES) such as kidney and liver. The in vitro tests confirmed that [email protected] actively killed 4T1 cells under laser irradiation, but the in vivo anti-tumor ability was needed to be tested. Hence, [email protected] was intravenously injected into the tumor-bearing mice. As shown in Figure 6C, the tumors of mice treated with PBS, laser or [email protected] show a similar trend to grow very rapidly, which rules out their individual role in tumor inhibition. In the group of mice injected with [email protected] followed by 635 nm laser irradiation (100 mW/cm2, 10 min), the combinational use showed significant inhibitory effect on tumors. Their tumor sizes were much smaller than that of the control and other treatment groups, and no recrudescence was noticed. The results suggested that the ALA molecules intratumorally released from [email protected] strengthened the in vivo PDT efficacy. Figure 6D shows that the mice have a steady weight growth for “[email protected] + laser” group, but no obvious change for “laser” group. For the control group, the mouse weight had a slight decrease. As observed in the hematoxylin and eosin (H&E) analysis (Figure 6E), major organs do not show distinct injury or inflammation. However, it was encouragingly observed that the damaged cells of the tumor after PDT treatment presented morphological characteristics greatly different from the control, and the majority of them were fragmented and disassembled.
Figure 6 (A) In vivo time-course fluorescence images of a 4T1 tumor xenografted mouse at pre-injection, 0.5, 1, 2, 4, 6, 8 and 10 h post-injection of [email protected] (B) Ex vivo fluorescence images of major organs (heart, liver, spleen, kidney, and lung) and the tumor collected at 10 h post-injection. (C) Tumor volume and (D) body weight of mice in various treatment groups over the experiment period. Data are presented in mean ± SD (n = 3 in each group). The Student’s t-test is carried out to compare the intensity of different organs (*p<0.05). (E) Histological H&E staining of major organs and tumors, magnification: ×400.
To sum up, we successfully prepared fluorescent Ag NDs in water using PPA as the capping/stabilizing agent. [email protected] emitted at ~640 nm with the QY of 2.1% and an average lifetime of ~5.1 ns. The attractive properties combining with ultrasmall size favored [email protected] to work well for both in vitro and in vivo fluorescence imaging. Moreover, [email protected] were biosafe and showed no cytotoxicity even at a high dosage. The positively charged polyLys-Cys-SH peptides were linked to [email protected] for electrostatic adsorption of ALA to synthesize [email protected] Without further functionalization, [email protected] efficiently accumulated in the tumors depending on passive targeting via the EPR effect. Under 635 nm laser irradiation, ALA released from [email protected] promoted the PDT efficacy against tumors. All the results proved that [email protected] was a powerful nanoplatform for tumor-targeted PDT.
The experiments are conducted according to the Guide for the Care and Use of Laboratory Animals published by NIH and approved by the Animal Ethics Committee, School of Medicine, Xi’an Jiaotong University, China.
This work was financially supported by Key Research and Development Projects in Shaanxi Province of China (2018ZDCXL-SF-01-02-01).
The authors report no conflicts of interest in this work.
1. Jin R. Quantum sized, thiolate-protected gold nanoclusters. Nanoscale. 2010;2(3):343–362. doi:10.1039/b9nr00160c
2. Lin CA, Yang TY, Lee CH, et al. Synthesis, characterization, and bioconjugation of fluorescent gold nanoclusters toward biological labeling applications. ACS Nano. 2009;3(2):395–401. doi:10.1021/nn800632j
3. Zheng J, Zhang C, Dickson RM. Highly fluorescent, water-soluble, size-tunable gold quantum dots. Phys Rev Lett. 2004;93(7):077402. doi:10.1103/PhysRevLett.93.077402
4. Zheng Y, Lai L, Liu W, Jiang H, Wang X. Recent advances in biomedical applications of fluorescent gold nanoclusters. Adv Colloid Interface Sci. 2017;242:1–6. doi:10.1016/j.cis.2017.02.005
5. Choi S, Dickson RM, Yu J. Developing luminescent silver nanodots for biological applications. Chem Soc Rev. 2012;41(5):1867–1891. doi:10.1039/C1CS15226B
6. Díez I, Ras RH. Fluorescent silver nanoclusters. Nanoscale. 2011;3(5):1963–1970. doi:10.1039/c1nr00006c
7. Petty JT, Story SP, Hsiang JC, Dickson RM. DNA-templated molecular silver fluorophores. J Phys Chem Lett. 2013;4(7):1148–1155. doi:10.1021/jz4000142
8. Das NK, Ghosh S, Priya A, Datta S, Mukherjee S. Luminescent copper nanoclusters as a specific cell-imaging probe and a selective metal ion sensor. J Phys Chem C. 2015;119(43):24657–24664. doi:10.1021/acs.jpcc.5b08123
9. Wang C, Wang C, Xu L, Cheng H, Lin Q, Zhang C. Protein-directed synthesis of pH-responsive red fluorescent copper nanoclusters and their applications in cellular imaging and catalysis. Nanoscale. 2014;6(3):1775–1781. doi:10.1039/C3NR04835G
10. Jia X, Li J, Han L, Ren J, Yang X, Wang E. DNA-hosted copper nanodots for fluorescent identification of single nucleotide polymorphisms. ACS Nano. 2012;6(4):3311–3317.
11. Tanaka S, Miyazaki J, Tiwari DK, Jin T, Inouye Y. Fluorescent platinum nanodots: synthesis, purification, characterization, and application to bioimaging. Angew Chem Int Ed. 2010;50:431–435. doi:10.1002/anie.201004907
12. Aikens CM. Electronic structure of ligand-passivated gold and silver nanodots. J Phys Chem Lett. 2001;2:99–104. doi:10.1021/jz101499g
13. Wilcoxon JP, Martin JE. Photoluminescence from nanosize gold clusters. J Chem Phys. 1998;108:9137. doi:10.1063/1.476360
14. Wu Z, Jin R. On the ligand’s role in the fluorescence of gold nanoclusters. Nano Lett. 2010;10(7):2568–2573. doi:10.1021/nl101225f
15. Knoppe S, Bürgi T. Chirality in thiolate-protected gold clusters. Acc Chem Res. 2014;47(4):1318–1326. doi:10.1021/ar400295d
16. Li G, Jin R. Atomically precise gold nanoclusters as new model catalysts. Acc Chem Res. 2013;46(8):1749–1758. doi:10.1021/ar300213z
17. Tsunoyama H, Sakurai H, Negishi Y, Tsukuda T. Size-specific catalytic activity of polymer-stabilized gold nanodots for aerobic alcohol oxidation in water. J Am Chem Soc. 2005;127(26):9374–9375. doi:10.1021/ja052161e
18. Santiago González BS, Rodríguez MJ, Blanco C, Rivas J, López-quintela MA, Martinho JMG. One step synthesis of the smallest photoluminescent and paramagnetic PVP-protected gold atomic clusters. Nano Lett. 2010;10(10):4217–4221. doi:10.1021/nl1026716
19. Sachan R, Ramos V, Malasi A, et al. Oxidation-resistant silver nanostructures for ultrastable plasmonic applications. Adv Mater. 2013;25(14):2045–2050. doi:10.1002/adma.201204920
20. Xie J, Zheng Y, Ying JY. Protein-directed synthesis of highly fluorescent gold nanoclusters. J Am Chem Soc. 2009;131(3):888–889. doi:10.1021/ja806804u
21. Russell BA, Jachimska B, Komorek P, Mulheran PA, Chen Y. Lysozyme encapsulated gold nanodots: effects of cluster synthesis on natural protein characteristics. Phys Chem Chem Phys. 2017;19:7228–7235. doi:10.1039/C7CP00540G
22. Yarramala DS, Doshi S, Rao CP. Green synthesis, characterization and antitumor activity of luminescent gold nanoparticles capped with apo-α-lactalbumin. RSC Adv. 2015;5:32761–32767. doi:10.1039/C5RA03857J
23. Wen F, Dong Y, Feng L, Wang S, Zhang S, Zhang X. Horseradish peroxidase functionalized fluorescent gold nanodots for hydrogen peroxide sensing. Anal Chem. 2011;83(4):1193–1196. doi:10.1021/ac1031447
24. Kong Y, Chen J, Gao F, et al. Near-infrared fluorescent ribonuclease-A-encapsulated gold nanoclusters: preparation, characterization, cancer targeting and imaging. Nanoscale. 2013;5(3):1009–1017. doi:10.1039/C2NR32760K
25. Guével XL, Hötzer B, Jung G, Hollemeyer K, Trouillet V, Schneider M. Formation of fluorescent metal (Au, Ag) nanodots capped in bovine serum albumin followed by fluorescence and spectroscopy. J Phys Chem C. 2011;115(22):10955–10963. doi:10.1021/jp111820b
26. Yu J, Patel SA, Dickson RM. In vitro and intracellular production of peptide-encapsulated fluorescent silver nanodots. Angew Chem Int Ed. 2007;46(12):2028–2030. doi:10.1002/anie.200604253
27. Granger M, Abadie B, Marchis-mouren G. Limited action of trypsin on porcine pancreatic amylase: characterization of the fragments. FEBS Lett. 1975;56:189–193. doi:10.1016/0014-5793(75)81088-X
28. Yao Y, Li N, Zhang X, et al. DNA-templated silver nanocluster/porphyrin/MnO2 platform for label-free intracellular Zn2+ imaging and fluorescence-/magnetic resonance imaging-guided photodynamic therapy. ACS Appl Mater Interfaces. 2019;11(15):13991–14003. doi:10.1021/acsami.9b01530
29. Yao Y, Zhao D, Li N, et al. Multifunctional Fe3O4@[email protected] molecular machine for magnetically targeted intracellular Zn2+ imaging and fluorescence/MRI guided photodynamic-photothermal therapy. Anal Chem. 2019;91(12):7850–7857. doi:10.1021/acs.analchem.9b01591
30. Zhang X, Xi ZQ, Machuki JO, et al. Gold cube-in-cube based oxygen nanogenerator: a theranostic nanoplatform for modulating tumor microenvironment for precise chemo-phototherapy and multimodal imaging. ACS Nano. 2019;13(5):5306–5325. doi:10.1021/acsnano.8b09786
31. Peng Q, Berg K, Moan J, Kongshaug M, Nesland JM. 5-Aminolevulinic acid-based photodynamic therapy: principles and experimental research. Photochem Photobiol. 1997;65(2):235–251. doi:10.1111/php.1997.65.issue-2
32. Peng Q, Warloe T, Berg K, et al. 5-Aminolevulinic acid-based photodynamic therapy: clinical research and future challenges. Cancer. 1997;79(12):2282–2308. doi:10.1002/(SICI)1097-0142(19970615)79:12<2282::AID-CNCR2>3.0.CO;2-O
33. Punjabi A, Wu X, Tokatli-apollon A, et al. Amplifying the red-emission of upconverting nanoparticles for biocompatible clinically used prodrug-induced photodynamic therapy. ACS Nano. 2014;8(10):10621–10630. doi:10.1021/nn505051d
34. AI-Kassas R, Donnelly RF, McCarron PA. Aminolevulinic acid-loaded Witepsol microparticles manufactured using a spray congealing procedure: implications for topical photodynamic therapy. J Pharm Pharmacol. 2009;61:1125–1135. doi:10.1211/jpp.61.09.0001
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