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Effect of Gold Nanoparticle Radiosensitization on Plasmid DNA Damage Induced by High-Dose-Rate Brachytherapy

Authors Yogo K, Misawa M, Shimizu M, Shimizu H, Kitagawa T, Hirayama R , Ishiyama H, Furukawa T, Yasuda H

Received 18 November 2020

Accepted for publication 19 December 2020

Published 14 January 2021 Volume 2021:16 Pages 359—370

DOI https://doi.org/10.2147/IJN.S292105

Checked for plagiarism Yes

Review by Single anonymous peer review

Peer reviewer comments 3

Editor who approved publication: Dr Thomas Webster

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Katsunori Yogo,1 Masaki Misawa,2 Morihito Shimizu,2 Hidetoshi Shimizu,3 Tomoki Kitagawa,3 Ryoichi Hirayama,4 Hiromichi Ishiyama,5 Takako Furukawa,1 Hiroshi Yasuda6

1Nagoya University Graduate School of Medicine, Nagoya, Aichi, Japan; 2Health and Medical Research Institute, National Institute of Advanced Industrial Science & Technology (AIST), Tsukuba, Ibaraki, Japan; 3Department of Radiation Oncology, Aichi Cancer Center Hospital, Nagoya, Aichi, Japan; 4National Institute of Radiological Sciences (NIRS), National Institutes for Quantum and Radiological Science and Technology (QST), Chiba-shi, Chiba, Japan; 5Graduate School of Medical Science, Kitasato University, Sagamihara, Kanagawa, Japan; 6Department of Radiation Biophysics, Research Institute for Radiation Biology and Medicine, Hiroshima University, Hiroshima, Japan

Correspondence: Katsunori Yogo
Nagoya University Graduate School of Medicine, 1-1-20 Daiko-Minami, Higashi-Ku, Nagoya, Aichi 461-8673, Japan
Tel +81 52 719 1103
Fax +81 52 719 3172
Email [email protected]

Purpose: Gold nanoparticles (AuNPs) are candidate radiosensitizers for medium-energy photon treatment, such as γ-ray radiation in high-dose-rate (HDR) brachytherapy. However, high AuNP concentrations are required for sufficient dose enhancement for clinical applications. Here, we investigated the effect of positively (+) charged AuNP radiosensitization of plasmid DNA damage induced by 192Ir γ-rays, and compared it with that of negatively (−) charged AuNPs.
Methods: We observed DNA breaks and reactive oxygen species (ROS) generation in the presence of AuNPs at low concentrations. pBR322 plasmid DNA exposed to 64 ng/mL AuNPs was irradiated with 192Ir γ-rays via HDR brachytherapy. DNA breaks were detected by observing the changes in the form of the plasmid and quantified by agarose gel electrophoresis. The ROS generated by the AuNPs were measured with the fluorescent probe sensitive to ROS. The effects of positively (+) and negatively (−) charged AuNPs were compared to study the effect of surface charge on dose enhancement.
Results: +AuNPs at lower concentrations promoted a comparable level of radiosensitization by producing both single-stranded breaks (SSBs) and double-stranded breaks (DSBs) than those used in cell assays and Monte Carlo simulation experiments. The dose enhancement factor (DEF) for +AuNPs was 1.3 ± 0.2 for SSBs and 1.5 ± 0.4 for DSBs. The ability of +AuNPs to augment plasmid DNA damage is due to enhanced ROS generation. While −AuNPs generated similar ROS levels, they did not cause significant DNA damage. Thus, dose enhancement using low concentrations of +AuNPs presumably occurred via DNA binding or increasing local +AuNP concentration around the DNA.
Conclusion: +AuNPs at low concentrations displayed stronger radiosensitization compared to −AuNPs. Combining +AuNPs with 192Ir γ-rays in HDR brachytherapy is a candidate method for improving clinical outcomes. Future development of cancer cell-specific +AuNPs would allow their wider application for HDR brachytherapy.

Keywords: gold nanoparticles, high-dose-rate brachytherapy, DNA damage, radiosensitization, 192Ir γ-rays, positively charged nanoparticles

Introduction

Recent advances in radiation therapy techniques have enabled the delivery of increased radiation doses to tumors. For example, a highly active 192Ir γ-ray source in high-dose-rate (HDR) brachytherapy delivers a higher and a localized dose to tumors within a shorter treatment time and with fewer fractions, than that by external beam therapy.1 Using a wire inside an implanted flexible catheter tube or solid tube, the Ir source is placed for treatment using an HDR treatment machine. The treatment machine can deliver the source remotely using computer-controlled methods (remote afterloading brachytherapy system).

Cervix cancer brachytherapy is an HDR brachytherapy that is used extensively in clinical settings and exhibits positive clinical outcomes. Several irradiation techniques and dose optimization methods have been developed over the past decade.2–6 Despite this, normal tissue injury, such as rectal tissue damage following radiation treatment of cervical cancer, still prevents the delivery of optimal doses, which is detrimental to treatment outcomes. Marginal recurrence often occurs around the radiated fields near the tumors where the availability of radiation tends to reduce such as in case of advanced cervical cancers. Thus, radiation sensitization agents that modify and enhance the local dose are necessary to deliver a sufficient dose to tumors, including its marginal regions.

Gold nanoparticles (AuNPs) are candidate radiosensitization agents for radiation therapy.7,8 AuNPs are particles with sizes on the nanometer scale. As with other high-Z materials, Gold (Au) is relatively safe for use in vivo. AuNPs cause dose enhancement by increasing photoelectric absorption, resulting in increased reactive oxygen species (ROS) generation.9 We propose a combination of HDR brachytherapy and AuNPs as a radiosensitizer, which can be an effective treatment against potential metastasis around primary lesions.

Previous studies on AuNP radiosensitization combined with radiation therapy mainly focused on the use of external beams, such as kV or MV X-rays.10–14 In the past few years, significant progress has been reported on the use of AuNPs combined with brachytherapy.15 These studies have proposed the substitution of the radioactive seeds (millimeter-sized) used in low-dose-rate brachytherapy with the injection of radioactive or non-radioactive AuNPs to enhance the effect of radiation. This treatment method has been named “nanobrachytherapy,” and is used for treating prostate cancer with low-energy photons such as 125I and 103Pd.

The dose enhancement effects by AuNPs are predicted to be larger for low-energy photons (optimal energy ~40 keV). However, the use of low-energy photons in radiation therapy is limited to the treatment of superficial tumors. Low-dose-rate (LDR) brachytherapy uses low-energy photons and can provide higher values of DEF compared with HDR sources.15 The use of an LDR source is rather limited in the current radiation therapy, such as in that for prostate cancers. In contrast, high-energy photons (MV X-rays from linear accelerators) are dominantly and widely used in the current radiation therapy. Despite this, the dose enhancement that occurs by using AuNPs with high-energy photons is predicted to be much smaller than that observed with lower energy photons. This study aimed to explore AuNP sensitization combined with HDR brachytherapy, which uses medium-energy photons. These photons are therefore predicted to achieve a better balance between clinical application and AuNP enhancement. Several studies on dose enhancement by AuNPs with HDR (192Ir) brachytherapy have been previously reported. Shahhoseini et al reported that the dose enhancement factor (DEF) for 1 mM (2% w/w) AuNPs with 15 nm was approximately 1.6 for cancer cell lines, as studied via cell survival assays.16 Physical dose enhancements by AuNPs in HDR brachytherapy were studied by Monte Carlo (MC) calculations in previous studies.17–19 Cho et al demonstrated a DEF of ~1.3 in tumors administered with 30 mg/g AuNPs, as determined by MC calculations.17 Lechtman et al revealed that the administration of ~100 mg/g AuNPs is necessary for tumors treated with 192Ir γ-rays to achieve a dose enhancement of double the prescribed dose.18 Zabihzadeh et al reported that the DEF was predicted to be approximately 1.2 upon administration of uniformly distributed AuNPs (30 mg/g).19 These studies using MC calculations revealed that a high concentration of AuNPs (10–100 mg/g) is necessary in tumors treated with 192Ir γ-rays, which is an unrealistic concentration for clinical cases. The 50% lethal dose (LD50) of ~3.2 g/kg has been reported for mice.7 Thus, the concentration of AuNPs necessary to produce significant dose enhancement must be reduced for clinical applications.

Radiation is known to injure cancer cells by triggering DNA damage. Therefore, revealing whether the AuNP affects radiation-induced events at the DNA level is an important step for clinical applications. For this purpose, plasmid DNA assays were widely performed.20–24 Merits of use of the plasmid include high sensitivity and easy detection of DNA damage. There are several studies on plasmid damage enhancement by AuNP with low-energy (kV) photons.20–24 However, the ability of AuNPs to sensitize cells to 192Ir γ-ray-induced DNA damage has not yet been studied. Dose enhancement by AuNPs is known to be dependent on photon energy and the energy spectrum. Previous studies have reported that the energy of photons has a major influence on the radiosensitizing power of AuNPs.7,8 The AuNPs sensitization on 192Ir γ-ray-induced DNA damage must be confirmed experimentally before clinical application, as the experimental data are limited compared to the studies on external beam therapy. Here, we investigated the effect of AuNP radiosensitization on plasmid DNA damage induced by γ-rays via HDR brachytherapy. We used 192Ir γ-rays with medium-energy photons (380 keV), which are clinically used in HDR brachytherapy to study DNA damage enhancement in terms of both single-stranded and double-stranded breaks. To reduce the concentration of AuNPs required, we used positively charged AuNPs to target negatively charged DNA. Furthermore, we studied the generation of ROS in the presence of AuNPs with fluorescent probes sensitive to ROS. The effects of positively (+) and negatively (−) charged AuNPs were compared to study the effects of the surface charge on dose enhancement.

Materials and Methods

Gold Nanoparticles and Characterization

Positively charged gold nanoparticles (+AuNPs) were prepared and synthesized through the chemical reduction of tetrachloroaurate (HAuCl4) in the presence of the 2-aminoethanthiol (AET) as described earlier.25 Briefly, a mixture of HAuCl4 and AET at a molar ratio of 1:1.5 was added to 0.1 mM sodium borohydrate (NaBH4) and reactions were terminated by adding 10 mM hydrogen peroxide. Following synthesis, the AuNPs were dialyzed to remove unreacted chemicals.

Positive charges were applied by modifying the AuNP surfaces with amine groups. +AuNPs were used at a final concentration of 64 ng/mL. We also used +AuNPs with a diameter of 1.4 nm (Cat# 2022, Nanoprobes, Yaphank, NY, USA). Negatively charged AuNPs (−AuNPs) with a diameter of 30 nm were also used (Cat#EM.GC30, British BioCell International Co. Ltd., Cardiff, United Kingdom). Negative charges were applied by citrate ligands, which remained after synthesis. It was comparable in terms of size and shape to AET. These negative charges realize stable dispersion of −AuNPs.

AuNPs were characterized using absorption spectroscopy (SynergyHTX, BioTek, VT, USA) and the dynamic light scattering method (ZetaSizer Nano-S, Malvern Instruments, Malvern, UK). In the spectrum, AuNPs produce a characteristic absorption peak around 530 nm. The height of the peak represents the size concentration of AuNPs.21 AuNPs were also observed by field emission scanning electron microscopy (FE-SEM) (S-4800, Hitachi High-Tech, Ibaraki, Japan). Zeta potentials reflecting the surface charge of the AuNPs were measured using ZetaSizer Nano-S. The concentrations of the AuNPs were analyzed by adding AuNP solutions to a glass tube and measuring the dry weight of colloids after evaporating the solutions. The concentration was independently measured by absorbance at 530 nm and was confirmed as being consistent with the weight measurements.

Plasmid DNA and Reagents

The 4.3-kbp pBR322 plasmid DNA (Cat# 319–00444, Nippon Gene Co., Ltd., Tokyo, Japan) suspended in Tris-ethylenediaminetetraacetic acid (TE) buffer was precipitated with ethanol to remove the buffer.26,27 The DNA in ultra-pure water was aliquoted and stored at –20°C until use. The DNA concentration was quantified by absorption at 260 nm using a spectrometer (NanoDrop, Thermo Fisher Scientific, Waltham, MA, US).

For irradiation using γ-rays in HDR brachytherapy, 500 ng DNA was mixed in 20 μL buffer with 64 ng/mL AuNPs and placed in a 0.5 mL polypropylene microtube. A low concentration of TE buffer (0.25 mM Tris, 0.025 mM ethylenediaminetetraacetic acid (EDTA), pH 7.5) was used for the subsequent DNA assays, as appropriate.21 Damage yields in the plasmid assay are highly dependent on the scavenging capacity of the prepared buffer. Tris buffer (0.25 mM) provided only a weak scavenging capacity. This buffer was selected to provide sensitivity to damage, allowing for radiation exposure via therapeutic HDR brachytherapy to be completed within a practical time period.

Irradiation Conditions

The sample tubes were fixed to a holder custom-made with water-equivalent plastics (Tough Water Phantom, Kyoto Kagaku Co., Ltd., Kyoto, Japan). The sample tubes were irradiated from the bottom under aerobic conditions with an 192Ir γ-ray at Aichi Cancer Center (Figure 1). An 192Ir source (Nucletron mHDR-v2, γ-rays; mean energy: 0.355 MeV; half-life: 73.81 days; dimensions: 3.5 mm × 0.6 mm) was driven into the catheters placed beneath the holder (Figure 1A). A single Ir source was connected to the wire driven using an HDR brachytherapy unit (microSelectron HDR-V3, Nucletron). The source moves in two tubes (brachytherapy applicator indicated in blue in Figure 1A), and stopped at different positions (indicated using yellow arrows), to provide a uniform dose. The delivered dose was controlled by the source positions and dwell times using the loading unit. Doses of 4–20 Gy were delivered to the samples.

Figure 1 Experimental setup. (A) Schematic and (B) photo of the plastic phantom for the sample holder and 192Ir source loading unit.

Dose calculations were performed with treatment planning systems (Oncentra v4.3, Nucletron) considering the thickness of the sample tube. Doses were delivered to cover the top of the DNA solution in the tubes with 4 Gy isodose lines located at ~10 mm from the 192Ir source and defined as the reference point.28,29 An air kerma strength of 26,810 cGy cm2 h−1 (U) was used, which corresponds to 242 GBq. A dose rate was approximately 5 Gy/min at the reference point.

The sample irradiations were performed within 2–3 hours on the same day. The samples were stored at 4°C until electrophoresis. The electrophoresis was performed within a few hours of irradiation.

Plasmid DNA Form Analysis

Breaks in the DNA were detected as form changes in the plasmids and quantified by subsequent electrophoresis on agarose gels. The native plasmid forms a supercoiled (SC) structure, similar to a small ring twisting. When DNA is irradiated, the phosphate backbone is cut, which results in the formation of single-stranded breaks (SSBs), SC plasmid was restructured into an open circular (OC) form, similar to a small ring relaxing and opening. If the phosphate backbone in both strands is excised, which results in the formation of double-stranded breaks (DSBs), the plasmid DNA changes into a linear (L) structure, like a single string. For this assay, two SSBs in proximity within approximately six base pairs were detected as an L structure.30 Samples were electrophoresed in 1% (w/v) agarose gel in TBE buffer (44.5 mM of Tris-borate with pH 8.4 and 1 mM of EDTA) at 25 V for 5 h at room temperature.21–33 The gels were stained with ethidium bromide (1 μg/mL) for over 20 h and washed with pure water for 1 h. The gel images were captured using a high-sensitive imager (ImageQuant LAS 4010, GE Healthcare, Chicago IL, US) under UV illumination. The fluorescence intensities of the three DNA bands were measured using an image analysis software (ImageQuant TL, GE Healthcare, Chicago IL, US). The intensity of the SC DNA bands was corrected by multiplying with a factor of 1.42, considering the differences in staining of the DNA forms.34 The ratios between the amounts of SC and L DNA forms and the total amount of DNA were quantified according to the intensity of each DNA band.

Calculation of SSB and DSB Yields

The chemical yields of SSBs and DSBs caused by 192Ir γ-ray irradiation were calculated as described previously.20,27 The SSB yield was calculated by fitting the data plotted as the logarithm of the fraction of SC plasmids as a function of the dose. The DSB yield was determined from the relationship between the fraction of L plasmids and the dose by fitting the data with a linear function. The SSB and DSB yields were derived by dividing each slope by the DNA mass (650 g mol−1 bp−1 × number of base pairs in the plasmid) and expressed in units of Gy−1 Da−1, where Dalton (Da) is equivalent to the atomic mass unit. The DEFs used to measure the radiation sensitization effect were calculated as follows: (break yield in tested AuNP solution)/(break yield in control without AuNPs).16,17,19,21 Statistical analysis was performed by conducting the Tukey–Kramer test. Values were considered statistically significant at P < 0.05.

Measurements of ROS Yield

The ROS yields by the AuNPs were measured with the fluorescent probe sensitive to ROS generation, as previously described.9 We used the fluorescent probe 2-[6-(4-amino) phenoxy-3H-xanthen-3-on-9-yl] benzoic acid (APF) (Sekisui Medical Co., Ltd., Tokyo, Japan, Excitation: 490 nm, Emission: 515 nm), which is particularly sensitive to hydroxyl radical (•OH). The samples with 10 μM fluorescent probe and 64 ng/mL AuNPs were placed in the sample tube. The samples were irradiated by the 192Ir γ-rays in the holder via the same procedure described for plasmid DNA irradiation. After irradiation, the brightness of the samples was measured with a plate reader (Synergy HTX, BioTek Instruments, Inc., VT, USA) and the results were compared. Quenching of APF by AuNPs in dispersion was not considered, because the concentration of APF was much higher than those of AuNPs in the assays.

Results

AuNP Characterization

We characterized the positively charged AuNPs synthesized in this study. The AuNP size, monodispersity, concentration, and Zeta potential were examined.

Figure 2A shows part of a TEM image of a synthesized +AuNP. The AuNP showed a generally circular shape and had a size of approximately 30 nm. Figure 2B shows the absorbance spectrum of the AuNPs for visible light. Characteristic absorbance peaks of around 530 nm were seen for synthesized 30 nm +AuNPs. The diameters were 27.7 ± 13.9 nm (mean ± SD) for synthesized +AuNPs and 32.9 ± 17.7 nm for −AuNPs. The diameter of the 1.4 nm (nominal) +AuNPs was found to be 64.4 ± 36.2 nm. This was much larger than the nominal size (1.4 nm), presumably due to aggregations. This was further confirmed via a TEM image of the 1.4 nm +AuNP (data not shown). The Zeta potentials were +30 ± 11.2 mV for synthesized +AuNPs and +14.9 ± 8.5 mV for 1.4 nm +AuNPs, respectively.

Figure 2 Characterization of positively charged gold nanoparticles (+AuNPs). (A) Transmission electron microscopy (TEM) image of 30-nm diameter +AuNPs, recorded at 400,000x magnification. Scale bar; 50 nm. (B) Absorbance measurement of 30-nm diameter +AuNPs at visible wavelengths, including the characteristic absorbance peak at around 530 nm.

Dose Distribution

Figure 3 shows the dose distribution for the sample tube stand on the holder: the 192Ir source was used and the dose was calculated via a treatment planning system. The top of the DNA solution in the tubes (~10 mm away from the source center) were covered with isodose lines of 4 Gy. The dose was uniformly delivered to the sample tubes. The dose deviations of each sample were within 6%. We irradiated DNA sample tubes as tumor targets, mimicking patient treatments. Dose delivery of HDR sources is much more localized and provides a higher dose than high-energy external beams; thus, the HDR source causes lesser side effects to normal tissues that surround the target, if the source is correctly placed in a planned position.

Figure 3 Dose distribution delivered around sample tube irradiated with 192Ir source. Dose distribution (4 Gy) is presented in color wash (red) from the front view (A) and the bottom view (B). Dose distribution was calculated with the treatment planning system.

Radiosensitization for Plasmid DNA Damage

Figure 4 shows the fraction of SC plasmid as a function of the delivered doses. The fraction of the SC plasmid decreased with the dose in the control group, indicating that γ-ray irradiation increased the occurrence of SSBs. In the presence of +AuNPs (both 1.4 nm and 30 nm), the decrease in the SC plasmid was much higher than that observed in the control group (without AuNPs). In contrast, the decrease in the SC plasmid in the presence of −AuNPs was not significantly different compared to that observed in the control group.

Figure 4 Supercoiled plasmid fraction as a function of radiation dose irradiated with the 192Ir source in the presence of gold nanoparticles (AuNPs).

Figure 5 shows the fraction of L plasmids as a function of the delivered dose. The fraction of L plasmids increased with the dose in the control, indicating an increase in DSBs as a result of γ-ray irradiation. This increase in DSBs was further increased in the presence of 30-nm diameter +AuNPs. Meanwhile, no significant changes were observed in the sample in the presence of −AuNPs and 1.4 nm +AuNPs. SSB and DSB yields, calculated as G values, were summarized for AuNPs (Table 1). These values were compared with those in the control group. The DEFs were also obtained for +AuNPs and −AuNPs relative to the control.

Table 1 Chemical Yields of Single (SSBs) and Double-Stranded Breaks (DSBs) in 192Ir-Irradiated Samples in the Presence of Gold Nanoparticles (AuNPs) and Corresponding Dose Enhancement Factors. Data are Presented as the Mean ± Standard Deviations from Three Independent Experiments

Figure 5 Linear plasmid fraction as a function of radiation dose irradiated with the 192Ir source in the presence of gold nanoparticles (AuNPs).

ROS Generation by AuNPs

Figure 6 shows the fluorescence intensity of APF as a function of radiation dose in the presence of AuNPs. APF intensity reflects ROS yields, particularly those of hydroxyl radicals (•OH) (9). ROS yields almost linearly increased with the delivered dose by 192Ir γ-rays. There were no significant differences between ROS yields in the presence of +AuNPs (30 nm) and −AuNPs (30 nm). However, ROS yields were considerably smaller in the presence of +AuNPs (1.4 nm) than AuNPs (30 nm).

Figure 6 Yields of reactive oxygen species (ROS) as a function of radiation dose irradiated with the 192Ir source in the presence of gold nanoparticles (AuNPs). ROS yields are evaluated as the fluorescence intensity of the fluorescent probe sensitive to ROS yields.

Discussion

Effect of Radiosensitization by +AuNPs on DNA Damage

SSB and DSB yields increased in plasmid DNA irradiated by 192Ir γ-rays in the presence of 30 nm +AuNPs (Figures 4 and 5). Plasmid damage yields appear to be highly dependent on the scavenging capacity of the preparation buffer, such as Tris.21 Variations in the fractions of SC and L DNA with dose are similar trends, as observed in previous DNA studies using the same buffer (0.25 mM TE) with 13 μg/mL AuNP and 25.6 keV X-rays.21 The increases observed in SSBs were similar for both 1.4 nm and 30 nm +AuNPs. In contrast, DSBs increased more in the presence of 30 nm +AuNPs than 1.4 nm +AuNPs (Figure 5).

+AuNPs exerted a radiosensitization effect on plasmid DNA damage induced by the 192Ir γ-rays used in HDR brachytherapy. As a result of 192Ir γ-ray irradiation in HDR brachytherapy, the DEFs were 1.3 for SSBs and 1.5 for DSBs for 30 nm +AuNPs, respectively (Table 1). The DEFs had relatively larger uncertainty because the DEFs were calculated from damage yields with/without AuNPs and suffered from error propagation of these values. Our data for SSB yield enhancement with medium-energy photons are comparable to values obtained by low-energy photons using the same buffer (0.25 mM Tris). The reported DEF was ~1.5 for SSBs using 160 kVp X-rays with 13 μg/mL (1.25 nM) and 11.9-nm diameter AuNPs.21 Our values are also comparable to those obtained by Butterworth et al using 160 kVp X-rays in Tris-EDTA buffer, which has more scavenging capacity than the buffer used in this study.20 Their results showed that the dose modifying factors were 2.12 (SSB) and 1 (DSB) for 50 μg/mL 20 nm AuNPs and 2.29 (SSB) and 1.25 (DSB) for 50 μg/mL 5 nm AuNPs. Brun et al reported that DEFs are 1.5–2.0 for SSBs in the presence of 20–40 nm AuNPs irradiated with 49 keV X-rays in water.22 Morozow et al reported that DEFs are 1.91–2.74 for SSBs in the presence of 26 nm AuNPs (2.4 mg/mL) irradiated with 100–200 kVp X-rays.23 All these previous works used non-functionalized AuNPs did not explicitly specify the surface charge of AuNPs used. These AuNPs presumably possess negatively charged due to citrate ligands, which remained after the synthesis. DEF for SSBs by +AuNPs was consistent with previously reported values obtained with −AuNPs. Foley et al used 5 nm +AuNPs and reported that dose enhancement ~2.1 at 1 Gy for SSBs by 100 keV X-rays.24 The DEFs obtained in this study are smaller than those obtained using low-energy X-rays. These results are consistent with the knowledge that lower energy photons interact with AuNPs through photoelectric absorption more than medium-energy photons and provide larger dose enhancement.

Burn et al reported that AuNP size dependency on the dose enhancement, as DEF for SSBs increased from 1.2 to 3.0 with the AuNP size increase, within a range of 8–92 nm in water.22 The trends were opposite to those reported by Butterworth et al in TE buffers.20 Our data of DEF for SSBs did not show a significant difference between 1.4 nm and 30 nm (Table 1). We think that the different trends observed in the three reports could be explained by the difference in experimental conditions, such as different solutions used in each assay.

The DEFs obtained via the plasmid DNA assays are close to the values reported for cell survival assays using the 192Ir source (HDR brachytherapy). Shahhoseini et al used 197 μg/mL AuNPs with 15 nm and reported a DEF of 1.54 for lung cancer cells and 1.67 for prostate cancer cells using the 192Ir source.16 Retif et al reviewed and summarized the dose modifying factors (reciprocal of DEF) for cell survival and discussed its photon energy dependence.8 Our data is also similar to that of the factors for cells using kV and MV X-rays, 2.4 μg/mL AuNP with 1.9 nm was used.14 The DEFs obtained in this study were similar to those predicted by MC calculations, which demonstrated a DEF of ~1.2 using 7–30 mg/mL AuNPs with 1.9 nm17 and 100 nm.19

It is notable that similar dose enhancement by +AuNPs was observed in this study. However, this dose enhancement was achieved using a much lower concentration of AuNPs. For comparison, the concentration of +AuNPs used in this study is approximately 200–3000 times lower than that used in previous DNA assays20,21 and cell survival assays,16 and six orders of magnitude lower compared with assumptions based on MC calculations.17,19

ROS Generation by AuNPs

ROS generation increased with the delivered dose of AuNPs (Figure 6). APF is known to be particularly sensitive to hydroxyl radicals (•OH), and fluorescence intensity is linearly proportional to [•OH].9 The ROS generation induced by 192Ir γ-rays is comparable to previously reported for 100 kVp X-rays.9 An increase in fluorescence intensity reflects increasing ROS in the presence of AuNPs.

The results for the 1.4 nm and 30 nm +AuNPs showed that AuNPs that generated higher amounts of ROS had a larger dose enhancement effect on DNA damage (Figure 5). An increase in SSBs and DSBs (ie dose enhancement by +AuNPs) could be explained by an increase in ROS generation by AuNPs irradiated with 192Ir γ-rays.

AuNP-induced ROS enhancement increases SSB and DSB yields. In contrast, the ROS yield of 1.4 nm +AuNPs is smaller than that of 30 nm +AuNPs at the same dose (Figure 6). These trends contradict previous findings that smaller AuNPs yield more ROS than larger AuNPs due to their larger surface area.9 However, previous findings are based on negatively charged AuNPs, which are much more stable against aggregations. There was a decrease in ROS yield when 1.4 nm +AuNPs were used, presumably due to AuNP aggregation. This was further confirmed via TEM images of 1.4 nm +AuNPs.

In contrast, the ROS yield did not differ between similarly sized AuNPs, such as 30 nm +AuNPs and of 30 nm −AuNPs. The amount of ROS generated by 192Ir γ-ray irradiation was similar for both 30 nm +AuNPs and 30 nm −AuNPs and was independent of the surface charge of the AuNPs.

Effects of Surface Charge of AuNPs

The surface charge of the AuNPs did not change the amount of ROS generated (Figure 6). While both +AuNPs and −AuNPs yielded similar levels of ROS, the extent to which they increased DNA damage differed. The DEF for 30 nm +AuNPs was 1.3 ± 0.2 for SSBs and 1.5 ± 0.4 for DSBs (Table 1). In contrast, there was no significant dose enhancement observed in the presence of −AuNPs, and damage yields were similar to those observed in the control group. Only the addition of +AuNPs promoted SSBs and DSBs in the plasmids.

We used similar sizes and concentrations of +AuNPs and −AuNPs, but their surface charges differed. The effect of AuNPs on radiation-induced DNA damage was, therefore, affected by the surface properties of the AuNPs. One possible explanation of these differences in DNA damage sensitization by these surface charges is given as follows: As DNA has a net negative charge, +AuNPs tend to be attracted and attach to the DNA. Binding of positive AuNPs to negative DNA was essential for dose enhancement. Accordingly, the interaction between DNA and +AuNPs, such as the binding and/or local increase of +AuNPs around the DNA, results in differences in DNA radiosensitization to radiation-induced damage compared to the radiosensitization induced by −AuNPs.

ROS were generated by the secondary electrons produced by the 192Ir γ-rays absorbed by the AuNPs. These electrons have enough energy to travel away from AuNPs and produce ROS. Thus, even though electrons have a negative charge, ROS generation is not affected by the surface charge of AuNPs.

MC calculations predicted that AuNPs would induce a DEF of ~1.2 in tumors treated with 192Ir γ-rays. However, these calculations assumed the use of very high concentrations of AuNPs (10–100 mg/g),17–19 which is an unrealistic concentration for clinical applications. Thus, a strategy to reduce the concentration of AuNPs while providing significant dose enhancement is necessary for their clinical application. In this study, +AuNPs were successfully used to considerably reduce AuNP concentrations by approximately three to six orders of magnitude, while providing similar dose enhancement. Our study, therefore, presents a promising strategy for increasing the local concentration of AuNPs around DNA by targeting DNA with positively charged AuNPs. We found that a low concentration of +AuNPs effectively promoted radiosensitization for DNA damage induced by 192Ir γ-rays. This radiosensitization occurred via an increase of the local concentration of +AuNPs around the DNA to a greater extent than −AuNPs.

We assume the use of +AuNPs with brachytherapy for the treatment of cervix cancer. For drug delivery, one of the strategies we suggest is the direct intratumoral injection of +AuNPs (sizes <10 nm) to the tumor volumes35,36 We think that this method provides specific accumulation in tumor cells while avoiding problems in blood circulation, such as renal excretion, capture in liver and spleen.37 In studies involving rat having glioma, intratumoral injection of 25 mg/mL AuNPs improved survival significantly, providing the concentrations of 5 mg/mL AuNPs in tumor.35 This amount of +AuNP could be synthesized by the methods adopted in our study. However, several limitations must be resolved to use +AuNPs in clinical applications.

Firstly, the usage of optimal sizes of +AuNPs needs further investigation. DNA binding ability of +AuNPs could be exploited and methods for their efficient delivery to the tumors should be studied.35 We think that 1.4 nm +AuNPs could be attracted by the DNA in vivo; however, 30 nm +AuNPs could not directly reach the DNA inside the cell nucleus. +AuNPs should be smaller than ~5 nm of the nuclear pore complex, which is present on the envelope of the cell nucleus and allows the transport of molecules.38 Thus, we think that the sizes of +AuNPs smaller than 5 nm would be preferable for future studies.

The second issue was the drug delivery of +AuNPs to targets.35 While +AuNPs target DNA, they should also target cancer cells and pass through the cell nucleus before reaching genomic DNA in clinical applications. We think that it is possible for bare +AuNP, without further modification, to reach the target cell. Cho et al reported that +AuNPs were adsorbed on the cell membrane (negatively charged) and showed a higher level (5–10 times) of uptake by the cell compared to −AuNPs.39 Interestingly, they suggested that +AuNPs can directly pass through the cell membrane without mediation by the endocytotic pathway.

Another method to deliver +AuNPs to cancer cells is by using liposomes: +AuNPs (size below 5 nm) are contained in liposomes, which causes an increase in uptake by the cell through endocytosis.40 Then, +AuNPs is released into the cytoplasm, and should then be transported to the nucleus of the cells to bind genomic DNA. This could be achieved by their affinity to DNA because of having a positive charge, or modifying the nuclear transportation signals on the surface of +AuNPs.40–42 Furthermore, multistage drug delivery systems are proposed, which change their physicochemical properties (such as size, surface charge) to achieve tumor penetration, enhanced cellular uptake, in response to the differences in the physiological blood circulation, tumor microenvironment, and intracellular environment.43

Thirdly, the stability of +AuNPs must be improved, especially for those with smaller sizes below 5 nm. +AuNPs are relatively unstable compared to −AuNPs. +AuNPs are known to be unstable, particularly in high salt conditions, and easily aggregate under physiological conditions. Thus, aggregation must be prevented, potentially via the modification of blocking reagents. Surface or amine group modifications are necessary to overcome or reduce these disadvantages caused by positive charges.

Conclusion

In this study, we investigated the ability of +AuNPs to enhance plasmid DNA damage induced by 192Ir γ-rays in HDR brachytherapy. +AuNPs promote a comparable level of radiosensitization to both SSBs and DSBs at lower concentrations than those used in cell survival assays and MC calculations. The ability of +AuNPs to promote plasmid DNA damage is due to enhanced ROS generation, such as •OH radicals. While, −AuNPs generated similar levels of ROS, they did not show significant DNA damage enhancement ability. Thus, dose enhancement by low concentrations of +AuNPs presumably occurred via binding DNA or increasing the local concentration around DNA. +AuNPs are effective candidate radiosensitizers that can be used in conjunction with HDR brachytherapy. Future development of surface modifications for improved stability and tumor delivery would generate methods that can more widely apply +AuNPs alongside therapeutic 192Ir γ-rays in HDR brachytherapy.

Abbreviations

AuNPs, gold nanoparticles; DEF, dose enhancement factor; DSB, double-stranded breaks; HDR, high-dose rate; MC, Monte Carlo; ROS, reactive oxygen species; SSB, single-stranded breaks; TEM, transmission electron microscopy.

Acknowledgments

This work was supported in part by JSPS KAKENHI Grant Numbers 25870707 and JP18K07679, the Program of the Network-Type Joint Usage/Research Center for Radiation Disaster Medical Science of Hiroshima University, and the NU-AIST alliance project. We are grateful to Saori Yamamoto, Mirano Kakinuma, and Takayuki Tsuchinoto from Kitasato University and Yuzuki Nishihara from Nagoya University for providing experimental support.

Disclosure

The authors declare no conflict of interests in this work.

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