1 January 2010 Photothermal therapy in a murine colon cancer model using near-infrared absorbing gold nanorods
Author Affiliations +
J. of Biomedical Optics, 15(1), 018001 (2010). doi:10.1117/1.3290817
The photothermal ablation of solid tumors using exogenous, near-infrared (NIR)-absorbing nanoparticles has been previously investigated using various preclinical models and is currently being evaluated in the clinic. Here, we evaluate the circulation kinetics, preliminary toxicity, and efficacy of photothermal ablation of solid tumors using gold nanorods systemically delivered and passively accumulated in a murine subcutaneous colon cancer model. Tumored animals were infused with nanorods followed by the percutaneous illumination of the tumor with an 808-nm laser. Control groups consisted of laser-only, nanorod-only, and untreated tumored animals. The survival of the treated and control groups were monitored for 60 days post-treatment. The survival of the photothermally treated group was statistically longer than the control groups, with approximately 44% tumor free through the evaluation period. Histopathology of the major organs of animals infused with nanorods did not indicate any significant toxicity at 60 days post-treatment. Particle biodistribution was evaluated by elemental analysis of the major organs of untumored mice at 1, 7, and 30 days after infusion with nanorods. Elemental analysis indicates nanorod clearance from the blood and retention by the reticuloendothelial system. This study indicates that gold nanorods are promising agents for photothermal ablation of solid tumors.
Goodrich, Bao, Gill-Sharp, Sang, Wang, and Payne: Photothermal therapy in a murine colon cancer model using near-infrared absorbing gold nanorods



The ablation of solid tumors has been investigated using a variety of energy methods, including endogenously absorbed laser energy1, 2, 3 and radio-frequency energy.4, 5 The tumor specificity of these approaches is generally limited by the precision of pretreatment imaging, the precision of applicator placement, and the energy-deposition shape of the applicator used (generally spherical or conical). As a result, the treatment of tumors surrounding or adjacent to critical structures is problematic, the possibility of residual positive margins may limit use, and the ablation of surrounding healthy tissue may result in cosmetically or medically unacceptable outcomes.

Recently, the use of submicron- or nano-sized particles has been investigated to provide a higher level of precision for ablative applications. The objective of particle-based therapy is to select or design the particle (by size, shape, or other properties) to specifically accumulate in the tumor and not in normal tissue. The particles can be delivered to the tumor either passively, accumulating in the tumor through vascular fenestrations (the enhanced permeability and retention effect, EPR),6, 7, 8 or actively targeted to receptors on tumor or tumor-vasculature cell surfaces.9, 10, 11, 12, 13, 14 The particle is then exposed to an external or proximate energy source to create a localized hyperthermia to ablate the tumor. The particle serves to transduce the applied energy into heat, and the selectivity of the accumulation of the particle in the tumor serves to focus the transduction at the desired target. It has been demonstrated in animal models that tumor-specific particle accumulation will provide tumor-specific ablation and minimize damage to adjacent tissue or structures.15 Particle-based localized hyperthermia has also been demonstrated to enhance the effects of radiation therapy by providing dose-enhancement proximate to the area of particle accumulation.16

Near-infrared (NIR) energy is an attractive energy source because human tissue and blood are minimally absorptive in these wavelengths. Particles that absorb near-infrared wavelengths will serve to transduce energy that would otherwise be dissipated. Additionally, commercially available lasers and fiber-optic delivery systems allow the minimally invasive, versatile delivery of energy to most tumor locations. A number of in vitro studies have been published using various near-infrared absorbing particles for tumor ablation, including nanocages,17, 18 nanoshells,11, 12 nanorods,19, 20, 21, 22, 23, 24, 25 and carbon nanotubes.10 The extension of this work into in vivo models was previously demonstrated by West using gold nanoshells26, 27 by El-Sayed 28 and von Maltzhan 25 using gold nanorods, and by Lu 29 using hollow nanoshells.

Recent theoretical evaluations of the thermal efficiency of gold nanorods have generated a significant interest in the use of these particles for photothermal applications because of their relatively small size and high theoretical absorption coefficients.30 However, one of the major concerns with gold nanorods has been the reported cytotoxicity of the surfactant cetyltrimethylammonium bromide (CTAB) used in the manufacture of the nanorods,31, 32, 33 and the nonspecific accumulation that may occur as a result of residual CTAB.34, 35 While there are previous studies of the biodistribution of gold nanorods36 and preliminary efficacy studies,25, 28 these reports do not evaluate the biodistribution, tumor accumulation, acute toxicity, and efficacy of photothermal ablation in a single study using one manufacturing process. One of the primary differences in the manufacturing process used in this report is the use of diafiltration to remove process residuals. Most published studies used centrifugation as the method for removing excess CTAB from the solution. However, centrifugation is a very costly method for the cleaning of the large volumes of materials that would be needed in a commercial therapy in humans. Diafiltration is easily scalable and can be used to process extremely large volumes of particles. In this work, we report the biodistribution of gold nanorods in healthy animals, the efficacy of photothermal treatment, and the toxicity of the particles at 60days post-infusion using material manufactured using this process.


Materials and Methods


Synthesis of PEGylated Gold Nanorods

HAuCl43H2O , CTAB, NaBH4 , AgNO3 , and ascorbic acid were purchased from Sigma-Aldrich and were used as received with no further modification or purification. Nanorods were synthesized using the method developed by Jana 37 with minor changes. In brief, gold seed particles were prepared by adding 250μL of 10mM HAuCl43H2O to 7.5mL of 100mM CTAB with brief, gentle mixing. 600μL of freshly prepared, ice-cold 10mM NaBH4 solution was added, followed by mixing for 2min . The nanorod growth solution was prepared by adding 40mL of 100mM CTAB, 1.7mL of 10mM HAuCl43H2O , and 250μL of 10mM AgNO3 followed by 270μL of 100mM ascorbic acid. To initiate nanorod growth, 840μL of the seed solution was added to the growth solution, mixed gently, and left still for 40min . Excess reactants were removed by centrifugation and resuspension in DI water. The size and distribution of the nanorods was evaluated by transmission electron microscope (TEM) [Fig. 1 ]. The nanorods were PEGylated by the addition of 1mM thiol-terminated methoxypoly(ethylene glycol) (mPEG-SH) (Laysan Bio) which was left to stir overnight. The final PEGylated rod solution was cleaned by diafiltration of the solution into DI H2O . After cleaning, the particles were transferred via diafiltration into a 10% (w/v) solution of trehalose to make the solution iso-osmotic with the blood. The final particles showed a strong plasmon resonance centered on 780nm [Fig. 1]. Residual CTAB content was estimated using elemental analysis of bromine content in the nanorod solution. Bromine content is an indirect measurement of the residual CTAB content of the solution. Using the measured concentration of bromine in the solution and assuming that each bromine is associated with a molecule of CTAB, it is possible to estimate the molar concentration of CTAB in the solution. Based on this number, we can estimate the solution concentration of CTAB at 3.2μgmL in the material used in these studies.

Fig. 1

(a) TEM image of gold nanorods used in this work. Average rod size was determined to be 44.7±5.4nm by 14.3±1.8 . Non-rod-shaped particles accounted for 10% of the particles observed. (b) The optical extinction spectrum of the nanorod particles used is shown in the right panel. All concentrations were standardized to an optical density at 800nm , the approximate laser wavelength used.



Animal Model and Inoculation with Tumor Cells

57 female Balb/c mice, 5to6weeks of age (Taconic, Hudson, New York ) weighing 16to20g were used in this study. For the tumor accumulation study, 9 animals were inoculated subcutaneously on the flank with 50μL ( 8×106cells per ml) of CT26.wt murine colon carcinoma (ATCC) suspended in PBS. For the photothermal efficacy study, 36 mice were inoculated subcutaneously on the flank with 50μL ( 8×106cell per ml) of CT26.wt murine colon carcinoma. Once the tumor reached a diameter of 7mm in any two directions, the animals were utilized. Of the 9 mice inoculated for the tumor accumulation study, 9 developed usable tumors. Of the 36 innoculated for the thermal efficacy study, 27 developed a treatable tumor. Twelve animals without tumors were used for the biodistribution studies. All animals were housed and all experiments were conducted in accordance with the Guide for Care and Use of Laboratory Animals in Nanospectra’s AAALAC-accredited animal facility.


Particle Biodistribution

At 1, 7, and 28days post-infusion, the animals were sacrificed, and the following tissues were collected for analysis: The brain, heart, lungs, kidneys, liver, spleen, and lymph nodes were taken in their entirety. Samples of the blood and bone were also collected for analysis. The tissue samples were weighed, placed in sample vials, and dessicated. The desiccated tissue, blood samples, or reference materials were analyzed by neutron activation analysis at the University of Texas at Austin (UT-Austin). This method has been shown previously to have sensitivity at 70picograms of Au per gram of tissue.38 Samples and gold standard solutions were placed in the rotary specimen rack of the Mark II TRIGA research reactor for 1h at 100kW . After a nominal one-week decay, the samples were counted in a close geometry using the Compton-suppression system. After counting, the samples were analyzed by UT-Austin for total gold content using a neutron activation analysis package.


Rate of Particle Accumulation in Tumor

Nine tumored mice were given an infusion via the tail vein of gold nanorods ( 4.5mlkg of 100 OD material). At each of the 16, 24, and 48h post-infusion time points, three mice were sacrificed. Their tumors were harvested, weighed, and dessicated prior to being sent for NAA analysis for gold content.


Photothermal Therapy

Twenty-four hours after a nanorod infusion, the animal was anesthetized with a combination of ketamine/xylazine/acepromazine. A cooled optical diffusing fiber with an isotropic diffusing tip of 1cm (LDF-10, BioTex, Inc., Houston, Texas ) was inserted percutaneously under the tumor, and an 808-nm laser (Diomed 15-plus, Diomed, Inc., Cambridge, UK ) was used to illuminate the tumor area for 180s at 3.5-W average power. A hypodermic needle thermocouple (HYP-1-30-1/2-T-G-60-SMP-M, Omega Engineering) was placed under the tumor and parallel to the laser fiber to measure the hyperthermia achieved, and the baseline body temperature was recorded using a rectal probe with a digital thermometer. Tumor size was measured three times weekly following therapy. Ellipsoidal tumor volume was calculated using the expression V=a*b*c*(π6) . For all groups, when tumors reached 500mm3 , animals were euthanized. Animals with a complete response were monitored for at least 60days after treatment.




Biodistribution of Infused Nanorods

To determine the biodistribution of the gold nanorods after infusion, 12 Balb/c mice received a tail vein infusion via catherization of PEGylated gold nanorods standardized to 6mLkg body weight at an optical density of 50 (approximately 6.5×1012 nanorods per ml). Other studies with mice of this strain, comparably sourced and housed, have demonstrated insignificant background gold content.38 At 1, 7, and 28days post-infusion, 4 mice were euthanized, and blood and major organs and selected tissue samples were harvested for neutron activation analysis. Figure 2 shows the percentage of total infused dose ( μg gold per tissue/total μg gold infused) in the major organs at 1, 7, and 28days post infusion. Figure 2 indicates that the organs of the reticuloendothelial system—the liver, spleen, and lymph nodes—had substantial nanorod accumulations. There was an insubstantial accumulation of gold in the lungs, kidney, heart, and brain.

Fig. 2

Gold content plotted as percentage of total infused dose at 1, 7, and 28days after nanorod infusion as measured by neutron activation analysis. Error bars represent the standard deviation in the measurement.



Nanorod Accumulation in Tumor

The gold nanorods are expected to accumulate in tumors through fenestrations in the vasculature of a rapidly growing tumor. The rate of particle accumulation will determine the optimal time for treatment post-infusion. To study the rate of particle accumulation in tumors, PEGylated gold nanorods were concentrated to an optical density of 100 and infused into the tail vein of nine tumored Balb/c mice at a dose of 4.5mLkg body weight (approximately 2×1013 nanorods per ml). Three animals per time point were sacrificed at 16h , 24h , and 48h after infusion. The tumor was extracted, desiccated, and submitted for neutron activation analysis along with a desiccated sample of the infused nanorod solution as a standard of gold content infused. The gold concentration in the tumor samples ( μg gold per gram of tumor) is shown in Figure 3 as a function of time after infusion. The mean gold concentration increases from 16hto24h by a factor of 1.8× . There is no significant increase in the gold concentration seen from 24hto48h post-infusion.

Fig. 3

Gold concentration in tumors in μg gold per gram of tissue after infusion with 4.5mLkg of 100 OD nanorods. Error bars represent the standard deviation in the measurement. Inset table shows the average tumor mass for each sacrifice point with the standard deviation.



Photothermal Therapy Treatment

Tumored animals were assigned randomly to four groups: nanorod-assisted photothermal therapy, N=9 ; nanorod-only (no laser application) control, N=7 ; laser-only (vehicle infusion, no nanorods) control, N=6 ; and untreated controls, N=5 . The photothermal therapy group received a tail vein infusion via catherization of PEGylated gold nanorods standardized to 6mLkg body weight at an optical density of 20 at 800nm (approximately 2.6×1012 nanorods per ml). The nanorod-only control group received a comparable tail vein infusion of nanorods as the treatment group, but no laser illumination. The laser-only control group received an infusion of the vehicle (10% trehalose) but no nanorods, and then a percutaneous laser illumination of the tumor similar to the treatment group. The untreated control group did not receive an infusion or laser application.

The temperature profiles of the nanorod-treated animals versus laser-only controls as measured by the hypodermic thermocouple inserted near the laser fiber are shown in Figure 4 . The average measured temperature in both groups increased during the 180-s treatment period. The average maximum temperature difference for nanorod-infused laser treated animals was 32.1°C±9.0°C . The average maximum temperature difference for the trehalose infused laser irradiated animals was 15.3°C±2.8°C . Based on the average subcutaneous temperature in a mouse of approximately 30°C , we observe a maximum temperature in tissue of 62±9.04°C for the nanorod-assisted therapy, and a maximum temperature in tissue in the laser-only control animals was 45.3°C±2.8°C .

Fig. 4

Thermal measurements in tissue proximal to the laser illumination site. The average value for the animals in each group is shown. The average maximum temperature difference for nanorod-infused laser-treated animals was ΔT=32.1°C±9.0°C . The average maximum temperature difference for the trehalose-infused laser-irradiated animals was ΔT=15.3°C±2.8°C .


The survival curve for all four groups is plotted in Figure 5 . The survival time comparison was augmented with a Kaplan-Meier survival analysis to generate confidence intervals for survival times.39 The mean survival time for the “no treatment” group was 8days , with a 95% confidence interval of 5.1to10.9days . The mean survival time for the “laser illumination only” group was 9.5days , with a 95% confidence interval of 7.7to11.3days . The mean survival time for the “nanorods only” group was 9.7days , with a 95% confidence interval of 6.3to13.1days . The mean survival time for the photothermal ablation group was 42.1days , with a 95% confidence interval of 30.3to53.9days . At day 60, 44% of the nanorod-treated mice that received a laser treatment survived, with evidence of a complete ablation of the tumor. The mean survival time of photothermally treated animals was statistically higher (p<0.001) than each control group. Survival of each control group was not statistically different from any other control group.

Fig. 5

Survival of tumor-bearing animals by treatment group. Survival of the treatment group was statistically significant from the control groups. The mean survival time for the “no treatment” group was 8days with a 95% confidence interval of 5.110.9days . The mean survival time for the “laser illumination only” group was 9.5days with a 95% confidence interval of 7.711.3days . The mean survival time for the “nanorods only” group was 9.7days with a 95% confidence interval of 6.313.1days . The mean survival time for the photothermal ablation group was 42.1days with a 95% confidence interval of 30.353.9days .



Histopathology of Nanorod-Infused Animals

Four animals showing complete tumor regression after nanorod infusion followed by laser illumination were sacrificed between 62 and 79days after infusion, and the major organs were collected for histopathology. Four animals that received nanorods but no laser treatment were sacrificed when their tumor volume exceeded limits (ranging from 8to18days after infusion), and the major organs were collected for histopathology. The major organs of three of the untreated controls were also submitted for histopathology for comparison. The tissues were blocked in paraffin, cut and stained using hemotoxylin and eosin (H&E). The stained slides were sent to be read by Dr. Charles Montgomery, DVM, DACVP, DACLAM (ComPath, Jay, Oklahoma). The following organs were examined histologically: brain, heart, lung, spleen, kidney, adrenal gland, mesenteric lymph nodes, and liver.

In all nanorod-infused animals, a “foreign body,” black in color and visible as single dots or aggregates of 5 to 50 dots, was observed in certain tissues. An example of the foreign body is shown in Figure 6 . In this image, the foreign body is visible in an H&E stained section of liver from an animal that received a nanorod infusion. Individual nanorods are too small to be seen under optical microscopy; therefore, the foreign bodies observed microscopically are believed to be accumulations or complexes of particles. The incidence, distribution, and grade of severity for inflammatory, degenerative, and proliferative lesions, as well as the presence of foreign bodies in tissues are shown in Table 1 .

Fig. 6

H&E stained liver section from an animal that received an i.v. infusion of Au nanorods. Arrows indicate the presence of the “foreign body” described in the pathology report. As individual nanorods are too small to be observed with optical microscopy, the foreign body is believed to be cluster of nanorods.


Table 1

Incidence, grade of severity and distribution of lesions in tissues.

Organ/lesionVehicle controlPhotothermal therapyNanorod control
Heart Mineralization00 2∕4 2.0 1∕4 1.0
Lung Chronic inflammation00 1∕4 1.0 1∕4 2.0
Spleen Acid hematin pigment 2∕3 1.0 4∕4 2.3 4∕4 1.0
 FB00 4∕4 1.0 3∕4 1.0
Kidney Mineralization0000 1∕4 1.0
Adrenal gland Subcapsular hyperplasia 3∕3 2.0 4∕4 1.0 1∕4 1.0
Mesenteric lymph node000000
LiverMononuclear cell infiltrate 2∕3 1.0 4∕4 1.0 2∕4 1.0
Chronic inflammation,etiology FB00 4∕4 1.0 4∕4 1.0
FB, sinusoids00 4∕4 1.0 4∕4 1.0

FB=foreign body. Grade of severity: 0=no lesion, 1=minimal , 2=mild , 3=moderate , 4=marked .

This foreign body was observed in the spleen (7 of 8) and liver (8 of 8) of the animals infused with nanorods. These foreign bodies were not observed in the brain, heart, lung, kidney, adrenal gland, or mesenteric lymph nodes. Splenic foreign bodies were located in the perifollicular zone of the lymphoid follicles and were minimal in severity. Liver foreign bodies were observed free in the sinusoids and occasionally in Kupffer cells lining the sinusoids. Chronic inflammatory lesions were observed in the liver associated with the presence of these foreign bodies, and these lesions consisted of infiltrates of lymphocytes, macrophages, and occasional plasma cells. These foci were random in distribution and minimal in severity, and were present in all of the nanorod-infused animals. This type of host response was not present in vehicle control animals.



The development of a clinically useful photothermal ablation technology must evaluate multiple questions. The particle must accumulate with sufficient selectivity in the tumor to confine thermal damage to the tumor, with minimal damage to surrounding healthy tissue. The accumulation rate of the particle in the tumor and the particle’s thermal transduction efficiency must be sufficient to allow transduction of an ablative level of energy. This applied energy must have minimal effect on tissue unless the transducing particles are present and must allow focal application to avoid damage to clearance organs such as the liver. Last, the infused particle dose must have a safety profile appropriate for the intended use (e.g., cancer in adults). The results of this study provide a preliminary answer to several of these questions.

It is important to note that broad generalizations regarding nanomaterials are problematic. For example, mean size, size distribution, shape, residual contaminants, and exponents may affect the safety or efficacy of any particular nanomaterial. Additionally, measurements of biodistribution should be evaluated in the context of the precision and direct/indirect nature of the measurement tool utilized. This study utilized gold nanorods approximately 14×45nm in size, and smaller or larger nanorods may have different tumor selectivity.

Particle accumulation in the tumor is perhaps the most important deciding factor in designing photothermal therapies. If the particle does not accumulate sufficiently using a particular injected dose to achieve ablative temperatures, the therapy can never be successful. Two important factors involved in the accumulation in tumor are the total particle dose and the rate of particle accumulation in the tumor. In order to determine the level of particle accumulation in this tumor model, accumulation studies were carried out using nanorod solutions concentrated to an optical density of 100 (approximately 2×1013 nanorods per ml). This concentration was chosen because it is comparable to the optical density of previous studies using gold nanorods.28 Tumors were harvested for gold analysis at 16h , 24h , and 48h after infusion. The gold accumulation was determined using NAA. NAA allows for the quantitative determination of gold in the evaluated tissue by comparison to a recognized standard, and has demonstrated sensitivity to 70picograms per gram.38 The results shown in Fig. 3 indicate that significant accumulation was achieved by 24h after infusion. This result is consistent with particle accumulations reported by El Sayed 28 As there was no significant increase in gold content measured after 24h , this time point was chosen for the photothermal therapy.

In any therapeutic treatment, it is desirable to use the least amount of exogenous material to achieve effective treatment. This is important both to keep the cost of a potential treatment low and to minimize any potential side effects due to the material in the body. A recent study of the thermal transduction efficiency of nanorods and other nanoparticles reports that the thermal transduction efficiency of the gold nanorods is approximately twice that of gold nanoshells for a given optical density.40 Based on measurements of gold accumulations from previous nanoshell studies15 and the estimated number of gold nanorods determined from the tumor accumulation levels using 100 optical density material, a therapeutically effective particle dose level, i.e., the minimum particle dose that would provide tumor accumulations adequate to achieve ablation, was estimated to be 6mLkg of particles concentrated to an optical density of 20. This dose level is significantly lower than that reported by El Sayed for their i.v. experiments (approx 5mlkg at 120 OD).28

The tumor accumulation studies indicate that there is a significant accumulation of particles in the tumor after a systemic infusion of gold nanorods. To successfully localize the thermal therapy to the tumor, it is also necessary to show selective accumulation in tumors. Our prior experience indicates that the presence of a tumor with a fenestrated vasculature does not materially alter biodistribution of infused particles among other organs because less than 10% of the total injected dose accumulates in the tumor. Accordingly, the biodistribution of infused nanorods was evaluated in nontumored animals. In addition, the use of nontumored animals would allow the biodistribution study to be extended to 28days post-infusion to get preliminary information about particle clearance from the body. The gold accumulation in various tissues was determined using NAA analysis and allows the harvest and measurement of whole organs but does not provide for intra-organ information. The results of this study indicate clearance and accumulation at 1, 7, and 28days after infusion by organs of the reticuloendothelial system, consistent with previous studies of other particles.36, 38 The largest accumulation of nanoparticles was observed in the liver and spleen, which together account for approximately 75% of the total injected nanoparticles at 1day post-injection. There was also a small accumulation of particles ( <1% total injected dose) seen in the kidney and lymph nodes. None of the other organs or tissues measured, including the heart, lungs, muscle, and bone show any significant gold content. The biodistribution indicates a gradual clearance of gold from the liver (72% of total dose at 1day to 62% of total dose at 28days ). While the gold content decreases in the liver over the 28-day study, the gold content in the other measured organs remains fairly constant. These biodistribution and tumor accumulation results indicate that nanorods of the present size will not extravasate into healthy tissue and must exit the blood stream through tumor vasculature fenestrations in order to be accumulated. As recently demonstrated, the use of different particle geometry (e.g., size, shape) tumor-specific targeting molecules may alter these kinetics, both within the tumor and in nontargeted organs.29

The success of a particle-assisted photothermal therapy depends on the particle accumulation and the appropriate laser dosimetry. Too high a laser exposure will cause excessive heating and damage to healthy tissue surrounding the tumor. If the laser dose is too low, then complete ablation may not be achieved, and the tumor may regrow. For this experiment, a laser exposure of 3.5-W average power for 180s was chosen, based on our previous studies using gold nanoshells.15, 27 In order to gauge the appropriateness of the chosen laser exposure using this particle and tumor model, the thermal response to laser treatment was measured for the two test groups subjected to thermal therapy via the use of a thermocouple inserted near the tumor site. The laser dosimetry of 3.5-W average power produced temperature rises sufficient to ablate the tumor proximate to the fiber placement. Observation of the tumors in the nanorod-treated mice that showed incomplete regression indicated that the tumor regrowth was from a location farthest from the placement of the optical fiber. As the thermal data illustrates that ablative temperatures were achieved in the nanorod-treated mice, this would indicate that the placement of the laser fiber may have affected the ablation of the tumors. In this study, we used a substantially lower particle dose than in the study by El-Sayed 28 While this combination of nanorod dose and laser exposure level was sufficient for ablative effects in all treated animals and a complete ablation in > 40% of the treated animals, further investigation of dose accumulations are warranted, particularly if safety thresholds will tolerate higher doses of particles.

This study also indicates encouraging results regarding the safety of a residual level of CTAB. CTAB been previously shown to be highly cytotoxic in solution31, 41 and unPEGylated CTAB-coated nanorods have also evidenced cytotoxic effects in cell culture.32 The use of PEG to displace the CTAB from the rod surface has been shown to reduce the observed toxicity of the particles in cell culture assays.32, 36, 43 However, cell culture toxicity assays generally focus on cell death at a 24-to72-h time points, which may be insufficient time for any residual CTAB to elute off the particle. The present biodistribution study indicates the presence of gold nanorods in the liver and spleen past 28days . The elemental analysis results indicate that nanorod-infused animals received approximately 0.32μg of CTAB per gram of body weight. The only significant lesion noted by the veterinary pathologist was a minimal incidence of chronic inflammation in the liver. We have observed in studies with gold nanoshells that do not contain CTAB a similar level of chronic inflammation in the liver, so we believe that this inflammation is not due to the levels of residual CTAB. While this inflammation appears to be minor, the presence of particles in the liver at 60days after infusion would suggest that a longer term chronic toxicity study would be warranted to determine any long-term effects of exposure to the nanorods. Histopathology did not indicate any significant lesions associated with the nanorod or residual CTAB levels.

This study demonstrates the safety and efficacy of the chosen gold nanorod for the photothermal ablation of solid tumors. The infused particles selectively accumulated in the tumor in quantities sufficient to provide significant ablation of the target lesions. There were no signs of acute toxicity from the infused particles through 60days after infusion. The results suggest that optimization of the particle dose and laser dosimetry may lead to a highly effective therapy. Further study of the long-term retention, clearance, and safety of the particles is required.


The authors would like to acknowledge the contribution of Dr. Jon Schwartz for his laser dosimetry work. The authors would also like to thank Dr. Charles Montgomery, DVM, DACVP, DACLAM of ComPath in Jay, Oklahoma, for performing the histopathology analysis. All authors were employees and equity holders of Nanospectra Biosciences during the performance of this study, and Nanospectra may benefit financially from commercialization of this work.



A. Carpentier, R. J. McNichols, R. J. Stafford, J. Itzcovitz, J. P. Guichard, D. Reizine, S. Delaloge, E. Vicaut, D. Payen, A. Gowda, and B. George, “Real-time magnetic resonance–guided laser thermal therapy for focal metastatic brain tumors,” Neurosurgery0148-396X 63(1), 21–28 (2008).Google Scholar


M. Kangasniemi, R. J. McNichols, J. A. Bankson, A. Gowda, R. E. Price, and J. D. Hazle, “Thermal therapy of canine cerebral tumors using a 980-nm diode laser with MR temperature-sensitive imaging feedback,” Lasers Surg. Med.0196-8092 35(1), 41–50 (2004).10.1002/lsm.20069Google Scholar


R. Puls, S. Langner, C. Rosenberg, K. Hegenscheid, J. P. Kuehn, K. Noeckler, and N. Hosten, “Laser ablation of liver metastases from colorectal cancer with MR thermometry: 5-year survival,” J. Vasc. Interv. Radiol.1051-0443 20(2), 225–234 (2009).10.1016/j.jvir.2008.10.018Google Scholar


G. S. Gazelle, S. N. Goldberg, L. Solbiati, and T. Livraghi, “Tumor ablation with radio-frequency energy,” Radiology0033-8419 217(3), 633–646 (2000).Google Scholar


A. N. Mirza, B. D. Fornage, N. Sneige, H. M. Kuerer, L. A. Newman, F. C. Ames, and S. E. Singletary, “Radio-frequency ablation of solid tumors,” Cancer J.1528-9117 7(2), 95–102 (2001).Google Scholar


O. Ishida, K. Maruyama, K. Sasaki, and M. Iwatsuru, “Size-dependent extravasation and interstitial localization of polyethyleneglycol liposomes in solid tumor-bearing mice,” Int. J. Pharm.0378-5173 190(1), 49–56 (1999).10.1016/S0378-5173(99)00256-2Google Scholar


H. Maeda, “The enhanced permeability and retention (EPR) effect in tumor vasculature: the key role of tumor-selective macromolecular drug targeting,” Adv. Enzyme Regul.0065-2571 41, 189–207 (2001).10.1016/S0065-2571(00)00013-3Google Scholar


H. Maeda, J. Fang, T. Inutsuka, and Y. Kitamoto, “Vascular permeability enhancement in solid tumor: various factors, mechanisms involved, and its implications,” Int. J. Immunopharmacol0192-0561 3(3), 319–328 (2003).10.1016/S1567-5769(02)00271-0Google Scholar


N. J. Durr, T. Larson, D. K. Smith, B. A. Korgel, K. Sokolov, and A. Ben-Yakar, “Two-photon luminescence imaging of cancer cells using molecularly targeted gold nanorods,” Nano Lett.1530-6984 7(4), 941–945 (2007).10.1021/nl062962vGoogle Scholar


N. W. S. Kam, M. O’Connell, J. A. Wisdom, and H. Dai, “Carbon nanotubes as multifunctional biological transporters and near-infrared agents for selective cancer cell destruction,” Proc. Natl. Acad. Sci. U.S.A.0027-8424 102, 11600–11605 (2005).10.1073/pnas.0502680102Google Scholar


C. Loo, A. R. Lowery, N. J. Halas, J. L. West, and R. Drezek, “Immunotargeted nanoshells for integrated cancer imaging and therapy,” Nano Lett.1530-6984 5(4), 709–711 (2005).10.1021/nl050127sGoogle Scholar


A. R. Lowery, A. M. Gobin, E. S. Day, N. J. Halas, and J. L. West, “Immunonanoshells for targeted photothermal ablation of tumor cells,” Int. J. Nanomed. 1(2), 149–154 (2006).10.2147/nano.2006.1.2.149Google Scholar


R. S. Norman, J. W. Stone, A. Gole, C. J. Murphy, and T. L. Sabo-Attwood, “Targeted photothermal lysis of the pathogenic bacteria, Pseudomonas aeruginosa, with gold nanorods,” Nano Lett.1530-6984 8(1), 302–306 (2008).10.1021/nl0727056Google Scholar


A. K. Oyelere, P. C. Chen, X. H. Huang, I. H. El-Sayed, and M. A. El-Sayed, “Peptide-conjugated gold nanorods for nuclear targeting,” Bioconjugate Chem.1043-1802 18, 1490–1497 (2007).10.1021/bc070132iGoogle Scholar


J. A. Schwartz, A. M. Shetty, R. E. Price, R. J. Stafford, J. C. Wang, R. K. Uthamanthil, K. Pham, R. J. McNichols, C. L. Coleman, and J. D. Payne, “Feasibility study of particle-assisted laser ablation of brain tumors in orthotopic canine model,” Cancer Res.0008-5472 64(4), 1659–1667 (2009).10.1158/0008-5472.CAN-08-2535Google Scholar


P. Diagaradjane, A. Shetty, J. C. Wang, A. M. Elliott, J. Schwartz, S. Shentu, H. C. Park, A. Deorukhkar, R. J. Stafford, S. H. Cho, J. W. Tunnell, J. D. Hazle, and S. Krishnan, “Modulation of in vivo tumor radiation response via gold nanoshell-mediated vascular-focused hyperthermia: characterizing an integrated antihypoxic and localized vascular disrupting targeting strategy,” Nano Lett.1530-6984 8(5), 1492–1500 (2008).10.1021/nl080496zGoogle Scholar


J. Y. Chen, D. L. Wang, J. F. Xi, L. Au, A. Siekkinen, A. Warsen, Z. Y. Li, H. Zhang, Y. N. Xia, and X. D. Li, “Immuno gold nanocages with tailored optical properties for targeted photothermal destruction of cancer cells,” Nano Lett.1530-6984 7, 1318–1322 (2007).10.1021/nl070345gGoogle Scholar


J. Y. Chen, B. Wiley, Z. Y. Li, D. Campbell, F. Saeki, H. Cang, L. Au, J. Lee, X. D. Li, and Y. N. Xia, “Gold nanocages: engineering their structure for biomedical applications,” Adv. Mater.0935-9648 17(18), 2255–2261 (2005).10.1002/adma.200500833Google Scholar


T. S. Hauck, T. L. Jennings, T. Yatsenko, J. C. Kumaradas, and W. C. W. Chan, “Enhancing the toxicity of cancer chemotherapeutics with gold nanorod hyperthermia,” Adv. Mater.0935-9648 20(20), 3832–3838 (2008).10.1002/adma.200800921Google Scholar


X. H. Huang, I. H. El-Sayed, W. Qian, and M. A. El-Sayed, “Cancer cell imaging and photothermal therapy in the near-infrared region by using gold nanorods,” J. Am. Chem. Soc.0002-7863 128(6), 2115–2120 (2006).10.1021/ja057254aGoogle Scholar


Y. F. Huang, K. Sefah, S. Bamrungsap, H. T. Chang, and W. Tan, “Selective photothermal therapy for mixed cancer cells using aptamer-conjugated nanorods,” Langmuir0743-7463 24(20), 11860–11865 (2008).10.1021/la801969cGoogle Scholar


T. B. Huff, L. Tong, Y. Zhao, M. N. Hansen, J. X. Cheng, and A. Wei, “Hyperthermic effects of gold nanorods on tumor cells,” Nanomedicine1743-5889 2(1), 125–132 (2007).10.2217/17435889.2.1.125Google Scholar


H. Takahashi, T. Niidome, A. Nariai, Y. Niidome, and S. Yamada, “Gold nanorod-sensitized cell death: microscopic observation of single living cells irradiated by pulsed near-infrared laser light in the presence of gold nanorods,” Chem. Lett.0366-7022 35(5), 500–501 (2006).10.1246/cl.2006.500Google Scholar


L. Tong, Y. Zhao, T. B. Huff, M. N. Hansen, A. Wei, and J. X. Cheng, “Gold nanorods mediate tumor cell death by compromising membrane integrity,” Adv. Mater.0935-9648 19(20), 3136–3141 (2007).10.1002/adma.200701974Google Scholar


G. von Maltzahn, J.-H. Park, A. Agrawal, N. K. Bandaru, S. K. Das, M. J. Sailor, and S. N. Bhatia, “Computationally guided photothermal tumor therapy using long-circulating gold nanorod antennas,” Cancer Res.0008-5472 69(9), 3892–3900 (2009).10.1158/0008-5472.CAN-08-4242Google Scholar


L. R. Hirsch, R. J. Stafford, J. A. Bankson, S. R. Sershen, B. Rivera, R. E. Price, J. D. Hazle, N. J. Halas, and J. L. West, “Nanoshell-mediated near-infrared thermal therapy of tumors under magnetic resonance guidance,” Proc. Natl. Acad. Sci. U.S.A.0027-8424 100(23), 13549–13554 (2003).10.1073/pnas.2232479100Google Scholar


D. P. O’Neal, L. R. Hirsch, N. J. Halas, J. D. Payne, and J. L. West, “Photo-thermal tumor ablation in mice using near infrared-absorbing nanoparticles,” Cancer Lett.0304-3835 209(2), 171–176 (2004).10.1016/j.canlet.2004.02.004Google Scholar


E. B. Dickerson, E. C. Dreaden, X. H. Huang, I. H. El-Sayed, H. H. Chu, S. Pushpanketh, J. F. McDonald, and M. A. El-Sayed, “Gold nanorod assisted near-infrared plasmonic photothermal therapy (PPTT) of squamous cell carcinoma in mice,” Cancer Lett.0304-3835 269(1), 57–66 (2008).10.1016/j.canlet.2008.04.026Google Scholar


W. Lu, C. Y. Xiong, G. D. Zhang, Q. Huang, R. Zhang, J. Z. Zhang, and C. Li, “Targeted photothermal ablation of murine melanomas with melanocyte-stimulating hormone analog-conjugated hollow gold nanospheres,” Clin. Cancer Res.1078-0432 15(3), 876–886 (2009).10.1158/1078-0432.CCR-08-1480Google Scholar


P. K. Jain, K. S. Lee, I. H. El-Sayed, and M. A. El-Sayed, “Calculated absorption and scattering properties of gold nanoparticles of different size, shape, and composition: applications in biological imaging and biomedicine,” J. Phys. Chem. B1089-5647 110(14), 7238–7248 (2006).10.1021/jp057170oGoogle Scholar


R. Cortesi, E. Esposito, E. Menegatti, R. Gambari, and C. Nastruzzi, “Effect of cationic liposome composition on in vitro cytotoxicity and protective effect on carried DNA,” Int. J. Pharm.0378-5173 139(1–2), 69–78 (1996).10.1016/0378-5173(96)04574-7Google Scholar


T. S. Hauck, A. A. Ghazani, and W. C. W. Chan, “Assessing the effect of surface chemistry on gold nanorod uptake, toxicity, and gene expression in mammalian cells,” Small1613-6810 4(1), 153–159 (2008).10.1002/smll.200700217Google Scholar


H. Takahashi, Y. Niidome, T. Niidome, K. Kaneko, H. Kawasaki, and S. Yamada, “Modification of gold nanorods using phosphatidylcholine to reduce cytotoxicity,” Langmuir0743-7463 22(1), 2–5 (2006).10.1021/la0520029Google Scholar


E. E. Connor, J. Mwamuka, A. Gole, C. J. Murphy, and M. D. Wyatt, “Gold nanoparticles are taken up by human cells but do not cause acute cytotoxicity,” Small1613-6810 1(3), 325–327 (2005).10.1002/smll.200400093Google Scholar


T. B. Huff, M. N. Hansen, Y. Zhao, J. X. Cheng, and A. Wei, “Controlling the cellular uptake of gold nanorods,” Langmuir0743-7463 23(4), 1596–1599 (2007).10.1021/la062642rGoogle Scholar


T. Niidome, M. Yamagata, Y. Okamoto, Y. Akiyama, H. Takahashi, T. Kawano, Y. Katayama, and Y. Niidome, “PEG-modified gold nanorods with a stealth character for in vivo applications,” J. Controlled Release0168-3659 114(3), 343–347 (2006).10.1016/j.jconrel.2006.06.017Google Scholar


N. R. Jana, L. Gearheart, and C. J. Murphy, “Wet chemical synthesis of high aspect ratio cylindrical gold nanorods,” J. Phys. Chem. B1089-5647 105(19), 4065–4067 (2001).10.1021/jp0107964Google Scholar


W. D. James, L. R. Hirsch, J. L. West, P. D. O’Neal, and J. D. Payne, “Application of INAA to the build-up and clearance of gold nanoshells in clinical studies in mice,” J. Radioanal. Nucl. Chem.0236-5731 271(2), 455–459 (2007).10.1007/s10967-007-0230-1Google Scholar


E. L. Kaplan and P. Meier, “Nonparametric estimation from incomplete observations,” J. Am. Stat. Assoc.0003-1291 53, 457–481 (1958).10.2307/2281868Google Scholar


J. R. Cole, N. A. Mirin, M. W. Knight, G. P. Goodrich, and N. J. Halas, “Photothermal efficiencies of nanoshells and nanorods for clinical therapeutic applications,” J. Phys. Chem. C1932-7447 113(28), 12090–12094 (2009).10.1021/jp9003592Google Scholar


C. L. Bean, S. M. Galloway, and M. O. Bradley, “Evaluation of three in vitro assays for assessment of membrane damage by surfactants,” In Vitro Toxicol. 4(2), 133–144 (1991).Google Scholar


H. Liao and J. H. Hafner, “Gold nanorod bioconjugates,” Chem. Mater.0897-4756 17, 4636–4641 (2005).10.1021/cm050935kGoogle Scholar

Glenn P. Goodrich, LiLi Bao, Kelly L. Gill-Sharp, Krystina L. Sang, James C. Wang, J. Donald Payne, "Photothermal therapy in a murine colon cancer model using near-infrared absorbing gold nanorods," Journal of Biomedical Optics 15(1), 018001 (1 January 2010). http://dx.doi.org/10.1117/1.3290817





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