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The quantitative sensitivity and dynamic range of conventional immunohistochemistry (IHC) with 3,3′-diaminobenzidine (IHC-DAB) used in pathological diagnosis in hospitals are poor, because enzyme activity can affect the IHC-DAB chromogenic reaction. Although fluorescent IHC can effectively increase the quantitative sensitivity of conventional IHC, tissue autofluorescence interferes with the sensitivity. Here, we created new fluorescent nanoparticles called phosphor-integrated dots (PIDs). PIDs have 100-fold greater brightness and a more than 300-fold greater dynamic range than those of commercially available fluorescent nanoparticles, quantum dots, whose fluorescence intensity is comparable to tissue autofluorescence. Additionally, a newly developed image-processing method enabled the calculation of the PID particle number in the obtained image. To quantify the sensitivity of IHC using PIDs (IHC-PIDs), the IHC-PIDs method was compared with fluorescence-activated cell sorting (FACS), a method well suited for evaluating total protein amount, and the two values exhibited strong correlation (R=0.94). We next applied IHC-PIDs to categorize the response to molecular target-based drug therapy in breast cancer patients. The results suggested that the PID particle number estimated by IHC-PIDs of breast cancer tissues obtained from biopsy before chemotherapy can provide a score for predicting the therapeutic effect of the human epidermal growth factor receptor 2-targeted drug trastuzumab.
Determining target protein expression levels in tissues is important for elucidating disease-associated mechanisms and categorizing the response to molecular target-based drug therapies. Various methods, including enzyme-linked immunosorbent assay (ELISA), fluorescence-activated cell sorting (FACS), and matrix-assisted laser desorption/ionization (MALDI), have been developed to quantify protein expression, and each has specific advantages. For example, FACS is a highly suitable method for assaying the total amount of protein present in cells. However, these methods cannot simultaneously evaluate both cellular morphology and properties that depend on protein expression levels1–5. Immunohistochemistry (IHC) enables the evaluation of both cellular characteristics6. In conventional IHC used in pathological diagnosis in hospitals, after the incubation of tissue sections with a primary antibody and a biotin-labeled secondary antibody, streptavidin-conjugated horseradish peroxidase (HRP) reacts with the secondary antibody, and this is followed by a chromogenic reaction of 3,3′-diaminobenzidine (DAB) with HRP7. Therefore, in IHC with DAB (IHC-DAB), the intensity of the DAB staining depends on the enzymatic activity of HRP and is significantly influenced by the reaction time, temperature and HRP substrate concentration. Consequently, the quantitative sensitivity of IHC-DAB is low.
Fluorescent labels are effective for increasing the quantitative sensitivity of IHC because the intensity of fluorescent materials is proportional to the intensity of the photon excitation energy7. Additionally, fluorescent labeling in conjunction with a dark background produces an image with a high signal-to-noise ratio. In previous studies, a fluorescence imaging system was developed using Cy-5 tyramide for compartmentalized, automated, quantitative analysis of histological sections (AQUA)8, 9. This method improved the quantitative sensitivity relative to IHC-DAB. However, general organic fluorescent molecules, such as FITC, Alexa Fluor, and Cy-5, have disadvantages, owing to their poor photostability and interference from tissue autofluorescence. In addition, signal amplification in the AQUA method occurs via enzymatic activity. Therefore, the AQUA method may leave a margin for improvement to allow for IHC with high quantitative sensitivity in clinical practice.
Recently, various types of fluorescent nanoparticles have been developed, including commercially available quantum dots (Qdots)10, 11, which exhibit greater photostability and brightness than general organic fluorescent molecules. However, tissue autofluorescence is strong and has an intensity comparable to Qdot fluorescence intensity. Therefore, in the presence of tissue autofluorescence, quantitative IHC-based analysis using only the fluorescence intensity of Qdots is challenging. We have recently developed a quantitative IHC-based analysis using Qdots (IHC-QDs) with an autofluorescence-subtracted image and single-particle Qdot imaging12, 13. For IHC-QDs analysis, we created a new optical system that combined a spinning disk confocal unit, electron multiplier charge-coupled device (EM-CCD) camera, and image processing12, 14–16. This optical system can be applied to various types of Qdot imaging applications intended for tissues (e.g., in vivo imaging14, 15). However, the produced system was not versatile. Most laboratories and pathology departments have only a normal optical microscope with a CCD camera, which is not sufficiently sensitive to detect single-particle Qdots. In addition, commercially available streptavidin-conjugated Qdots possess only 5–10 streptavidin molecules on their surface, thereby suggesting a low reactivity of Qdots with biotin-labeled secondary antibodies. Thus, most scientists and pathologists have high expectations that the fluorescence intensity and reactivity of nanoparticles to target proteins could be enhanced significantly over the corresponding values for Qdots.
To substantially mitigate these problems of IHC with fluorescent nanoparticles by using a versatile optical system, we created organic fluorophore assembly-conjugated nanoparticles suitable for IHC called phosphor-integrated dots (PIDs). The PIDs possess three main properties: (I) 100-fold greater fluorescence intensity relative to Qdots; (II) high photostability, owing to the densely packed fluorophores obtained through networked chemical binding of the fluorophores; and (III) hyper-reactivity, owing to the 2,460-molecule streptavidin-supported surface structure, which provides a dynamic range more than 300-fold greater than that of Qdots. Additionally, we developed an image-processing method to calculate the particle number of PIDs on images acquired by using a versatile optical system. Using these three characteristics of PIDs and image processing, we developed a quantitative diagnostic imaging system to measure the expression levels of target proteins on tissues on the basis of the number of PID particles. In fact, when the quantitative sensitivity of IHC using PIDs (IHC-PIDs) was compared with that of FACS, the two methods exhibited strong correlation. Moreover, the IHC-PIDs enabled quantitative estimation of the expression level of human epidermal growth factor receptor 2 (HER2), which plays a crucial role in breast cancer. The HER2 imaging data revealed that the PID particle number provides a remarkably accurate score for predicting the effect of HER2-targeted molecular drug therapy, thus suggesting that IHC-PIDs can dramatically improve the diagnostic capability of various molecular-targeted drug therapies.
We have previously developed organic fluorophore (tetramethylrhodamine)-assembly-conjugated nanoparticles (TMR nanoparticles) for IHC17. The fluorescence intensity of the TMR nanoparticles was 10-fold greater than that of the Qdots. However, because the fluorescence intensity of the TMR nanoparticles did not greatly exceed the tissue autofluorescence, we could not exclude the effect of autofluorescence interference17. In the present study, we prepared approximately 100,000 perylene diimide assembly-conjugated nanoparticles, called PIDs, for use in IHC (Fig. 1a). The PID particles were uniform in size (Fig. 1b) and had an average size of 149nm (Fig. 1b,c). Fluorescence spectral analysis demonstrated that the 580nm light-excited spectral patterns of the perylene diimide and PID particles peaked at approximately 620nm (Fig. 1d). The 580nm light-excited fluorescence intensity of the PID particles was approximately 100-fold greater than that of Qdot 625 (Fig. 1e), which exhibited fluorescence intensity comparable to the autofluorescence intensity. This result suggested that the PID fluorescence was significantly stronger than the tissue autofluorescence. The PIDs also possessed much greater photostability than that of perylene diimide (Fig. 1f). The 580nm light-excited fluorescence intensity of perylene diimide rapidly decreased to 2% over 10min, whereas the fluorescence intensity of the PIDs remained at a value greater than 80% under the same irradiation conditions. The photostability of the PIDs is attributable to the dense packing of the perylene diimide, owing to both the networked chemical binding of perylene diimide and the use of a capsule to protect the perylene diimide from oxidization. Moreover, a single PID has approximately 2,460 streptavidin molecules linked via polyethylene glycol (PEG) chains on its surface (Fig. 1a and Supplementary Fig. 1), whereas a single streptavidin-conjugated Qdot possesses only 5–10 streptavidin molecules. Therefore, PIDs are expected to exhibit significantly higher reactivity to the secondary antibody. In addition, although the PIDs have many streptavidin groups on the surface of a single nanoparticle, the density of streptavidin on the PIDs surface is comparable to that of streptavidin-conjugated Qdots. There are varieties of Qdots that possess different emission properties from short (e.g. Qdot 525) to long wavelength (e.g. Qdot 655). The Qdot number indicates the emission wavelength in nm. The emission wavelength of a Qdot shifts from short to long wavelength with increasing particle size. The form and size of Qdot 525 and Qdot 655 excluding surface PEG chains were observed by transmission electron microscopy18. From this information, we estimated the surface area of Qdot 525 and Qdot 655 to be 58.1nm2 and 349.6nm2, respectively. Streptavidin-conjugated Qdots have 5–10 streptavidin molecules linked via PEG chains on their surface. Thus, in Qdot 525 and Qdot 655, when five streptavidin molecules are conjugated, the density of streptavidin in a single Qdot is one streptavidin molecule per approximately 11.6 to 69.9nm2. Similarly, when ten streptavidin molecules are conjugated, the density of streptavidin in a single Qdot is one streptavidin molecule per approximately 5.8 to 35.0nm2. The total range of area for a single streptavidin molecule in Qdot 525 and Qdot 655 is about 5.8 to 69.9nm2. On the other hand, the surface area of a single PID is 70,650nm2. Since the number of streptavidin molecules in the PID is 2,460, the density of streptavidin in a single PID is one streptavidin molecule per approximately 28.7nm2, falling in the middle of the range calculated for Qdot 525 and Qdot 655. Thus, the streptavidin density in PIDs is comparable to that of established technology.
Our image-processing method included three steps: (step I) identification of a bright spot arising from PID fluorescence and not from noise; (step II) definition of the area of a bright spot derived from PIDs; and (step III) estimation of the number of PID particles in the bright spot. Prior to steps I–III, the input fluorescence image (Fig. 2a) was high-pass filtered to remove autofluorescence and noise (Fig. 2b) because the bright spot of the PID fluorescence contained more high-frequency components than the background fluorescence and noise.
First, in step I, all regions of the high-pass-filtered image (1,600×1,200 pixels) were scanned using a matrix filter of 3×3 pixels to identify a local maximum point (Figs 2d and and3a).3a). Local maximum points were identified when the center pixel value was higher than the 8 surrounding pixel values (Figs 2d and and3b).3b). Similarly, local minimum points were identified when the center pixel value was less than the 8 surrounding pixel values (Figs 2c and and3c).3c). Therefore, no local maximum points or minimum points were observed when the distribution of the brightness values gradually changed (Fig. 3b,c). A merged image was created that showed both types of points (Fig. 2e). To identify the local maximum point that resulted from the bright spot of the PID fluorescence, the region around each local maximum point was searched for the nearest local minimum point (Fig. 3d). The difference between the brightness of the local maximum point value and its corresponding local minimum point was determined as a comparison (Fig. 3d). If the brightness value difference between the local maximum point and the corresponding local minimum point was less than 32 (in the 12-bit image), the local maximum points were ignored as false-positive points (Fig. 3d). We called the threshold value the “noise tolerance”. The local maximum points over the noise tolerance were adopted as bright spots that resulted from PIDs (Figs 2f and and3d).3d). By properly setting the noise tolerance, we confirmed that the positive bright spots resulting from the PIDs were detected in fluorescence microscopy images with high accuracy (F-measure, F=0.90).
Second, in step II, the high-pass-filtered images were binarized using a threshold of 16 (in the 12-bit image) (Fig. 2g), and the bright spot areas were determined (Fig. 2h). The images obtained in steps I and II were integrated (Fig. 2i) to determine positive spots that resulted from the PID signal and their areas. If the spots observed in Fig. 2h did not exist in the positive points identified in Fig. 2f, the bright spot area was ignored. The brightness values of the positive bright spots in Fig. 2i were then converted to the number of PID particles in the next step (step III).
Third, in step III, to investigate the relationship between the fluorescence intensity and the particle number in a bright spot, we simultaneously imaged PID bright spots in human cancer tissues using fluorescence to measure the fluorescence intensity of each bright spot (Fig. 2j,l) and scanning electron microscopy (SEM) to count the PID particle number of each bright spot (Fig. 2k,l). Various patterns derived from many positive bright spots (n=443) were analyzed using both imaging methods. The fluorescence signals (Fig. 2j) were analyzed using the same method as in steps I and II, and then the particle number was determined using SEM images (Fig. 2k). Both scores were used to generate a standard curve (Fig. 2m) with a high correlation between the fluorescence signals and the PID particle number (correlation coefficient, R=0.98). The combination of steps I, II, and III enabled the identification of positive bright spots and the estimation of the number of PID particles per bright spot.
Various concentrations of biotin solution were applied to a deparaffinized section of human breast cancer tissue to prepare a mimic slide. After incubation with biotin molecules, the non-bonded free biotin on the mimic slides was washed off. Streptavidin-conjugated HRP, streptavidin-conjugated Texas Red, and streptavidin-conjugated Qdots or PIDs were reacted with the biotin-bonded slide glass and observed. Streptavidin-conjugated HRP was visualized with DAB and analyzed with an Aperio image analysis system (Leica) to quantify the degree of brown coloring from IHC-DAB. Other samples were observed using a versatile fluorescence microscope with a normal CCD camera. The effective dynamic ranges of DAB, Texas Red, and Qdot staining were 10−5 to 10−3 (Fig. 4a), 10−4 to 3×10−2 (Fig. 4b), and 10−4 to 10−2mM (Fig. 4c), respectively. By contrast, the effective dynamic range of the PIDs was 10−6 to 10−1mM (Fig. 4d,e). Thus, of all the staining methods, PID staining produced the broadest dynamic range, from very low to fairly high. In addition, on the mimic slides incubated only with phosphate-buffered saline (PBS) lacking biotin (Fig. 4e, 0mM condition), the PID particle number was 8.8 in 0.01mm2 (100μm×100μm square). The size of a cell is defined as a 10-μm square, so there are 100 cells in the 100μm×100μm area. Therefore, an 8.8 PID particles in 0.01mm2 (Fig. 4e, 0mM condition) corresponds to about 0.09 PID particles in a cell. These data indicate that non-specific binding of PIDs to cancer tissues is very weak.
Next, the measurement quantitative sensitivity of IHC-PIDs was investigated using cultured cells of eight types of breast cancer. First, the HER2 expression levels of these cells were examined using FACS. FACS is not suitable for diagnosis of pathology specimens for which observation of cellular morphology and characteristics is needed. However, because FACS uses a small fluorescent dye molecule, among existing techniques it is a highly suitable method for assaying the total amount of proteins present in fixed cells. Consequently, the correlation with FACS was used to determine whether our technique was capable of assaying protein expression level in a pathology specimen with high accuracy. Each type of cell was fixed with formalin and then labeled with an anti-HER2 antibody and a secondary antibody conjugated to Alexa Fluor 488. We measured the fluorescence intensity per cell by FACS (n=20,000)19 and then calculated the mean number of HER2 proteins per cell by using a standard curve. SK-BR3 cells exhibited the highest expression level of HER2, with approximately 5×104 proteins per cell (Fig. 4f, x-axis). These results suggest that the actual number of HER2 proteins that can be recognized by the anti-HER2 antibody is approximately 5.0×104, owing to the effect of formalin fixation, although the number of HER2 proteins in living SK-BR3 cells is known to be 2.0×106 per cell20. Next, paraffin sections of these cultured cells were immunostained with a monoclonal anti-HER2 antibody and a monomerized and biotinylated monoclonal secondary antibody, and PIDs and were observed using a versatile fluorescence microscope (Fig. 4g). The obtained fluorescence data were analyzed via the newly developed image-processing method (Figs 2 and and3)3) to determine the number of PID particles per cell. The mean number of PIDs per cell (Fig. 4f, y-axis) was then calculated and compared with the value determined by FACS (Fig. 4f, x-axis). The two values exhibited strong correlation (R=0.94) (Fig. 4f), thus demonstrating that IHC-PIDs can measure the protein expression level in cells with high accuracy.
Trastuzumab is a humanized monoclonal antibody against HER221. In clinical practice, HER2 gene amplification and protein overexpression have been measured by fluorescence in situ hybridization (FISH) and IHC-DAB. IHC-DAB against HER2 is classified into only 4 categories (scores of 0, 1, 2, and 3); furthermore, these categories are not based on quantitative amounts of HER protein. According to the recommended practice guideline for HER2 testing, negative for HER2 is defined as IHC-DAB scores of 0–1+, equivocal for HER2 is defined as IHC-DAB scores of 2+, and positive for HER2 is defined as IHC-DAB scores of 3+. In cases of score 2+, FISH is required to judge whether HER2 positive or negative22. Recently, neoadjuvant chemotherapy with trastuzumab has been administered to HER2-positive patients23. When the HER2 status of breast cancer tissues obtained from biopsy before chemotherapy and surgery is categorized as score 3 in HER2 testing by IHC-DAB or over score 2.0 in HER2 testing by FISH, anthracycline, a topoisomerase inhibitor, is administered for three months and is followed by trastuzumab and taxanes, paclitaxel, or docetaxel, which are microtubule inhibitors, for three months24. After treatments, if surgically removed cancer tissues do not exhibit invasive cancer cells and lymph-node metastasis, the patients are defined as having a pathologic complete response (pCR)25. By contrast, if the cancer tissues have invasive cancer cells and/or lymph-node metastasis, the patients are defined as having a non-pathologic complete response (non-pCR)25. We acquired tissues obtained from biopsy before chemotherapy from 74 HER2-positive patients who received neoadjuvant chemotherapy (Supplementary Table 1). These tissues were examined by IHC-DAB (Fig. 5a,e), FISH or IHC-PIDs (Fig. 5b–d,f–h). The staining intensity of IHC-DAB was analyzed using Aperio image analysis (Fig. 5i). The tissues of patient nos. 12 and 67 both had a HER2 score of 3 by IHC-DAB and a FISH score of approximately 6. The DAB intensities of patient no. 12 (score, 98.4) and no. 67 (score, 89.1) analyzed using Aperio image analysis were similar. However, patient no. 12 had pCR, and patient no. 67 had non-pCR. The staining results from 74 HER2-positive patients suggest that IHC-DAB (Fig. 5i, p=0.210) and FISH (Fig. 5j, p=0.521) were unable to distinguish between cases of pCR (n=34) and non-pCR (n=40). By contrast, IHC-PIDs distinguished pCR (n=34) from non-pCR (n=40) with statistical significance (p=0.0272) (Fig. 5k).
In clinical practice, hematoxylin-eosin (HE) staining is the most widely used method to visualize cellular morphology, and pathologists use information about cellular morphology to diagnose cancer cell behavior, on the basis of their clinical experience. Therefore, to perform pathological diagnosis with high accuracy, simultaneous observation of both cellular morphology and properties using a single tissue section would be beneficial. However, simultaneous observation of these properties is difficult for the following two reasons: (I) the brown color of DAB staining is similar to the red color of eosin staining, thus hindering their differentiation; and (II) the fluorescence intensity of eosin is far superior to that of Qdots, thus making it difficult to observe a fluorescent dye or Qdot on an eosin-stained sample. However, the fluorescence intensity of PIDs is higher than that of eosin. Thus, we detected the PID signal (Fig. 6a,c) on samples stained with HE (Fig. 6b,c) and clearly observed the atypical nuclei and cell shapes. Therefore, this method enabled us to evaluate both the cellular morphology and properties in a single tissue sample.
In this study, IHC-PIDs analysis of cultured human breast cancer cells and tissues was performed using a fluorescence microscope manufactured by the Olympus Corporation. To provide more evidence of the versatility of IHC-PIDs, we sought to perform PID imaging using versatile microscopes from other companies. We measured the HER2 expression levels of eight types of cultured cancer cells, shown in Fig. 4g, as the number of PID particles number per cell by using fluorescence microscopes from Zeiss and Keyence. Then, the correlation between the data obtained using fluorescence microscopes from Olympus and Zeiss (Fig. 6d) and Olympus and Keyence (Fig. 6e) was evaluated. For these measurements, a BX53 fluorescence microscope (Olympus) with a DP73 CCD camera (Olympus), an Axio Imager Z1 fluorescence microscope (Zeiss) with an AxioCam CCD camera (Zeiss), and a BZ-X700 fluorescence microscope (Keyence) with a BZ-X710 CCD camera (Keyence) were used. The data obtained using the Zeiss (Fig. 6d) and Keyence (Fig. 6e) microscopes were significantly correlated with the data for the Olympus microscope (both with correlation coefficients R>0.98), thus demonstrating that the IHC-PIDs method enables accurate measurement of protein expression levels independently of the optical system.
As part of interdisciplinary translational research integrating nanotechnology and clinical pathology, in this study we created new fluorescent nanoparticles called PIDs that have 100-fold greater fluorescence intensity than that of Qdots. Qdot brightness is not sufficient to completely avoid interference from autofluorescence because of the comparable intensity of tissue autofluorescence. In contrast, PID fluorescence was significantly stronger than the tissue autofluorescence and was able to produce an image with a high signal-to-noise ratio in the presence of autofluorescence.
A newly developed image-processing method enabled the calculation of the PID particle number in a bright spot of the obtained image by using a versatile optical system with high accuracy. Therefore, our IHC-PIDs method can identify a single PID that recognizes a target molecule quantitatively in IHC under a versatile optical system. Importantly, the fluorescence signal should be measured not as the PID fluorescence intensity, but as the PID particle number in a cell or a defined area in tissues. The fluorescence intensity of the PIDs changes depending on the specific configuration of the optical system. However, the particle number of PIDs is an absolute value and does not vary across systems. In this study, we obtained IHC-PIDs data by using primarily a normal fluorescence microscope manufactured by the Olympus Corporation. Because the number of PID particles per cell determined using the Zeiss and Keyence normal fluorescence microscopes was significantly correlated with the Olympus data, the IHC-PIDs method is a versatile optical technique that can estimate accurate protein expression levels independently of the optical system.
Figure 4 shows that the dynamic range of IHC-PIDs (10−6 to 10−1mM) was 1,000-fold and more than 300-fold greater than that of DAB (10−5 to 10−3mM) and a fluorescent probe (Texas Red, 10−4 to 3×10−2mM; Qdots, 10−4 to 10−2mM), respectively. PID imaging notably exhibited high sensitivity at low biotin concentrations. The high sensitivity over a greater dynamic range of IHC-PIDs is thought to be useful for accurate assessment of low-level biomolecular changes. During signal transduction, local modification or expression of proteins can play pivotal roles in important cell functions. Therefore, the detectability of target modifications or expression that occurs at low levels can have a strong effect on IHC-based studies and diagnoses.
PID staining enabled simultaneous imaging of cellular morphology and properties in a single tissue section stained with HE and PIDs (Fig. 6a–c). For the pathological section (2–4μm thickness), we prepared two adjacent sections that were mirror images of each other. However, the thickness of the blade edge of the microtome used to prepare the section was approximately 1.5μm, on the basis of the SEM image (data not shown). Therefore, even if two adjacent sections are mirror images, there is a gap of 1.5μm between the two sections because this thickness of tissue is eliminated by the edge of the microtome. Therefore, it is challenging to observe an identical cross-sectional surface in two adjacent sections. Because we observed cellular morphology and properties in true identical sections using HE and PIDs staining, we believe that IHC-PIDs will be useful for performing cancer mechanism study and pathological diagnosis with high accuracy.
We successfully used IHC-PIDs of a biopsy sample to distinguish pCR and non-pCR of neoadjuvant chemotherapy with trastuzumab performed before chemotherapy and surgery. Knowledge of the diagnostic results before chemotherapy might allow doctors to modify the treatment regimen for patients who are expected to experience non-pCR by adding or substituting other HER2-targeted drugs with different mechanisms of action (e.g., pertuzumab26, T-DM127, lapatinib28, or neratinib28). Therefore, we believe that IHC-PIDs might be used to select the anti-tumor effects of anticancer agents and thus benefit cancer patients. Additionally, because this new method enhances the therapeutic selectivity of drugs and promotes therapeutic efficiency of drug use, this method is expected to sharply reduce healthcare costs.
First, 16.5mg of perylene diimide29 (Tokyo Chemical Industry, Tokyo, Japan) and 100mg of Emulgen (Kao, Tokyo, Japan) were dissolved in 18.5mL of distilled water. Then, the solution was stirred and heated at 70°C. Next, 0.78g of methylol melamine (Nippon Carbide Industries, Tokyo, Japan) and 980μL of 10% dodecylbenzenesulfonic acid aqueous solution (Kanto Chemical, Tokyo, Japan) were added to the solution and heated at 65°C for 30min. After an additional 50min after the 30minutes at 65°C, the solution was heated at 75°C for 20min. To wash the obtained perylene diimide-conjugated nanoparticles, the dispersion was centrifuged, and the supernatant was discarded. Distilled water was added to the sample and dispersed using a UH-50 ultrasonic homogenizer (SMT, Tokyo, Japan), and the sample was further washed using ethanol and distilled water. The obtained perylene diimide assembly-conjugated nanoparticles were then subjected to surface modification.
First, 20mg of 1,2-bis(2-aminoethoxy)ethane (Tokyo Chemical Industry) was added to the dispersion of the perylene diimide assembly-conjugated nanoparticles and heated at 70°C for 20min to modify the amino groups. Next, 15mg of NHS- PEG-MAL (Thermo Fisher Scientific, Tokyo, Japan) was added to the dispersion of the amino-modified perylene diimide assembly-conjugated nanoparticles and stirred at 20°C for 1h. To wash the obtained MAL-PEG-modified fluorescent nanoparticles, the dispersion was centrifuged at 10,000×g for 20min, and the supernatant was discarded. The sample was dispersed in distilled water using an ultrasonic homogenizer. 2-Iminothiolane HCl was added to 1mL of a solution of 0.01mg of streptavidin (Nacalai Tesque, Kyoto, Japan), stirred for 60min, and then purified using a column to obtain thiolated streptavidin. The thiolated streptavidin was added to the dispersion of the MAL-PEG-modified perylene diimide assembly-conjugated nanoparticles to obtain streptavidin-modified fluorescent nanoparticles (PIDs). The dispersion was washed four times using PBS, and the PIDs were dispersed using 1% bovine serum albumin (BSA) in PBS. The number of streptavidin molecules on the PIDs was calculated from the streptavidin concentration measured using the BCA method (Pierce, Thermo Fisher Scientific, Tokyo, Japan) (Supplementary Fig. 1). The measurements indicated that the surface of a single PID was attached to approximately 2,460 streptavidin molecules via PEG chains.
The excitation and emission wavelengths of perylene diimide and PID particles in PBS were investigated using a spectrometer (F-7000, Hitachi, Tokyo, Japan). The 580nm light-excited fluorescence intensity of perylene diimide, Qdot 625 (Thermo Fisher Scientific; the number indicates the emission wavelength) or PID particles was examined using an F-7000 spectrometer. The fluorescence intensities of a single molecule of perylene diimide, a single Qdot 625 particle, and a single PID particle were calculated and compared. To examine the photostability of the perylene diimide and PIDs, each was irradiated with 580nm light, and the fluorescence intensities were measured over time using a BX53 fluorescence microscope (Olympus, Tokyo, Japan) with a UPLSAPO objective lens 40×2 (40×, 0.95 NA, Olympus) and a DP73 CCD camera (Olympus).
To examine the dynamic range of IHC-PIDs, mimic slides coated with various concentrations of biotin were imaged. Paraffin sections of human breast cancer tissue (US Biomax, MD, USA) were deparaffinized in xylene and hydrated with a graded alcohol series and distilled water. The samples were incubated with 10−6, 10−5, 3×10−5, 10−4, 3×10−4, 10−3, 3×10−3, 10−2, 3×10−2, or 10−1mM NHS-PEG-biotin (Thermo Fisher Scientific) at 25°C for 1h. This treatment caused the NHS-PEG-biotin to bind to the tissue sections. After a PBS wash, the samples were incubated with 1% BSA in PBS at 25°C for 10min for blocking. The samples were washed and treated with streptavidin-conjugated HRP (I-VIEW DAB Universal kit, Roche, Tokyo, Japan), 20μg/mL streptavidin-conjugated Texas Red (Vector Laboratories, CA, USA), 40nM streptavidin-conjugated Qdot 625 particles (Thermo Fisher Scientific) or 0.05nM PIDs at 25°C for 1h. The concentrations of streptavidin-conjugated HRP, Texas Red, and Qdot 625 were as recommended in the manufacturer’s instructions. After being washed with PBS, all samples were dehydrated and mounted in mounting medium for observation. For this observation, the focal point was the interstitial area in the tissues, which were imaged with an optical microscope (BX53, Olympus) using a UPLSAPO 40×2 (Olympus) objective lens and CCD camera (DP73, Olympus). The sample stained with streptavidin-conjugated HRP was treated with DAB (I-VIEW DAB Universal Kit, Roche), observed with a bright field microscope, and analyzed using the Aperio image analysis system (Leica, Tokyo, Japan). The samples stained with streptavidin-conjugated Texas Red, streptavidin-conjugated Qdot 625 particles or PIDs were observed through a fluorescence filter (64HE, Zeiss, Tokyo, Japan). Four microscopic fields in each sample were observed, and the mean values were obtained.
Cultured breast cancer cells (1.5×107 cells) were fixed in 10% neutral buffered formalin mixed with alginic acid solution. The sample was embedded with alginate gel and treated with paraffin to prepare a paraffin block using a dedicated device (Retratome REM-700, Yamato Kohki, Saitama, Japan). The samples were cut into 3μm thick sections and mounted on glue-coated glass slides.
All paraffin sections were deparaffinized in xylene and hydrated in a series of graded alcohols and distilled water. Antigen retrieval was performed by boiling the samples in 10mM citrate buffer (pH 6.0) for 40min at 98°C. Then, the samples were immunostained with the monoclonal antibody 4B5 (Roche) at 25°C for 40min. The samples were washed with PBS and then incubated with 6μg/mL biotinylated secondary antibody. Before incubation with the secondary antibody, the anti-rabbit monoclonal antibody (LO-RG-1, Bio-Rad, CA, USA) was monomerized through a reduction reaction. The antibody monomerization exposed the thiol group of the hinge region in the antibody, which was biotinylated using Biotin Labeling Kit-SH (Dojindo, Kumamoto, Japan). After incubation with the biotinylated secondary antibody at 25°C for 30min, the sample was treated with 0.02nM PID at 25°C for 1h. The sample was washed, stained with hematoxylin and mounted in mounting medium (multimount480, Matusnami, Osaka, Japan). The PID fluorescence signals were observed using fluorescence microscopy (BX53, Olympus) with a UPLSAPO 40×2 (Olympus) objective lens and CCD camera (DP73, Olympus) in 5 microscopic fields (with 1,000 cells investigated in each sample).
Cultured breast cancer cells were fixed in 10% formalin, and the samples (2×106 cells) were mixed with PBS containing 5% fetal bovine serum, 1mM EDTA, and 0.1% NaN3. The samples were immunostained with 5μg/mL primary antibody to HER2 (Anti-C-ErbB2/c-Neu(Ab-5) Mouse mAb(TA-1), Calbiochem, Merck Millipore, Tokyo, Japan) at 4°C for 30min. After a PBS wash, the samples were incubated with 1μg/mL secondary antibody (Anti-Mouse IgG-Alexa Fluor488, Abcam, Tokyo, Japan) at 4°C for 30min. After a PBS wash, the samples were mixed with dedicated buffer for FACS and subjected to FACS measurements (MACSQuant Analyzer, Miltenyi Biotec, Bergisch Gladbach, Germany). We measured the fluorescence intensity per cell of 20,000 cells by FACS19 and calculated the mean value. Fluorescence-labeled beads (QIFIKIT) were also measured for calibration. QIFIKIT is used to determine the density of antibody-binding antigen per cell using FACS.
We identified 6,824 patients with primary invasive breast cancer who underwent surgery at the Department of Surgery, Tohoku University Hospital (Sendai, Japan), Iwate Prefectural Central Hospital (Morioka, Japan), Tohoku Kosai Hospital (Sendai, Japan), Miyagi Cancer Center Hospital (Natori, Japan), Nihonkai General Hospital (Sakata, Japan), Osaki Citizen Hospital (Osaki, Japan), or Japanese Red Cross Ishinomaki Hospital (Ishinomaki, Japan) between January 2007 and December 2013. We selected 74 HER2-positive breast cancer specimens from 89 patients who were treated with neoadjuvant chemotherapy with trastuzumab. The pathological response of the surgically resected tumor was evaluated after neoadjuvant chemotherapy. A pathological complete response (pCR) was defined as the absence of all invasive cancer cells and lymph node metastasis, regardless of the presence or absence of noninvasive cancer cells25. We used samples from 34 pCR and 40 non-pCR patients that were obtained from a biopsy before neoadjuvant chemotherapy.
The Ethical Committees of the Graduate School of Medicine at Tohoku University, Iwate Prefectural Central Hospital, Tohoku Kosai Hospital, Miyagi Cancer Center Hospital, Nihonkai General Hospital, Osaki Citizen Hospital, and Japanese Red Cross Ishinomaki Hospital approved this protocol. Before performing IHC and FISH in this study, we obtained informed consent from all the patients. All patients signed an Ethical Committee consent form and agreed to serve as tissue donors for the experiments. The methods were conducted in accordance with the approved guidelines.
HER2 testing by IHC-DAB was performed with a kit for IHC-DAB (HercepTest, Dako, CA, USA). The results of IHC-DAB were scored by two pathologists as follows: score 0 represents no staining or incomplete membrane staining in 10% or less of tumor cells; score 1 represents incomplete membrane staining in more than 10% of tumor cells; score 2 represents weak to moderate complete membrane staining in more than 10% of tumor cells or complete membrane staining in 10% or less of tumor cells; and score 3 represents intense circumferential membrane staining in more than 10% of tumor cells22. The DAB-stained sample was also analyzed with an Aperio image analysis system (Leica). FISH was conducted using a PathVysion HER2 DNA Probe Kit (Abbott, IL, USA). The slides were hybridized with probes to HER2/neu and the centromere marker CEP17. The ratio of HER2 genes to CEP17 genes was determined (ECLIPSE Ni, Nikon, Tokyo, Japan). A FISH score of 2.0 or greater indicated a HER2-positive sample.
All breast tumor tissue specimens were fixed in 10% neutral buffered formalin and embedded in paraffin according to standard procedures. The samples were cut into 3μm thick sections and placed on glue-coated glass slides. The subsequent processes were performed in the same manner as the IHC of the paraffin sections of cultured human breast cancer cells.
In this study, S-4800 (Hitachi) was used for scanning electron microscopy (SEM).
In this study, an Axio Imager Z1 (Zeiss) fluorescence microscope with a CCD camera (AxioCam, Zeiss), a BX53 microscope (Olympus) with a CCD camera (DP73 Olympus), and a BZ-X700 microscope (Keyence, Tokyo, Japan) with a CCD camera (BZ-X710, Keyence) were used for IHC. An ECLIPSE Ni microscope (Nikon) with a CCD camera (Ds-Qi1Mc, Nikon) was used for FISH.
All data are presented as the mean±s.e.m. F-tests were performed, and equal variance was defined as a p-value (p)≥0.05. Comparisons between groups were performed using parametric Student’s t-tests (p≥0.05 in the F-test) or Welch’s t-tests (p<0.05 in the F-test). A value of p<0.05 was considered significant for both t-tests.
We thank M.Mukai and T.Natori for technical assistance. We also acknowledge support from the Biomedical Research Core at the Tohoku University Graduate School of Medicine. A portion of this work was supported by a Grant-in-Aid for Scientific Research (B) (16H05168) and Exploratory Research (16K15572) from the Japan Society for the Promotion of Science (K.G.); a Grant-in-Aid for Scientific Research in Innovative Areas “Nanomedicine Molecular Science” (23107009) from the Ministry of Education, Culture, Sports, Science, and Technology, Japan (K.G.); a Grant-in-Aid for the Comprehensive Research and Development of an Early Stage Diagnosis Method and Instruments to Treat Cancer from the New Energy and Industrial Technology Development Organization, Japan (K.G., M.W., H.T., M.M., H.O., Y.N., and N.O.); and a Grant-in-Aid for The A3 Foresight Program from the Japan Society for the Promotion of Science, Japan (K.G. and N.O.).
K.G. conceived and designed the project, designed and performed experiments and conducted the data analysis. H.T., M.M., T.K., T.I., S.U., H.H., Y.K., Y.H., R.Y., A.F., and N.O. removed tissue samples and selected human tissue samples. M.W., H.T., M.M., and Y.T-A. prepared the sections. K.G., M.W., Y.T.-A., H.O., H.G., H.N., M.T., and Y.N. designed a method for staining the PIDs. M.W., H.T., and M.M. analyzed the clinical data and discussed the results. K.G., H.O., H.G., K.T., H.N., M.T., and Y.N. developed the PIDs. Y.O. and Y.Y. wrote the software. K.G., M.W., H.T., M.M., Y.N., and N.O. directed the project. K.G. wrote the manuscript.
The authors declare that they have no competing interests.
Electronic supplementary material
Supplementary information accompanies this paper at doi:10.1038/s41598-017-06534-z
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