1. Cell Biology
  2. Immunology and Inflammation

Functional visualization of NK cell-mediated killing of metastatic single tumor cells

  1. Hiroshi Ichise
  2. Shoko Tsukamoto
  3. Tsuyoshi Hirashima
  4. Yoshinobu Konishi
  5. Choji Oki
  6. Shinya Tsukiji
  7. Satoshi Iwano
  8. Atsushi Miyawaki
  9. Kenta Sumiyama
  10. Kenta Terai
  11. Michiyuki Matsuda  Is a corresponding author
  1. Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Japan
  2. Department of Pathology and Biology of Diseases, Graduate School of Medicine, Kyoto University, Japan
  3. Department of Nanopharmaceutical Sciences, Nagoya Institute of Technology, Gokiso-cho, Japan
  4. Brain Science Institute, Center for Brain Science, RIKEN, Hirosawa, Japan
  5. Laboratory for Mouse Genetic Engineering, RIKEN Center for Biosystems Dynamics Research, Japan
  6. Institute for Integrated Cell-Material Sciences, Kyoto University, Japan
https://doi.org/10.7554/eLife.76269
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Cite this article
  1. Hiroshi Ichise
  2. Shoko Tsukamoto
  3. Tsuyoshi Hirashima
  4. Yoshinobu Konishi
  5. Choji Oki
  6. Shinya Tsukiji
  7. Satoshi Iwano
  8. Atsushi Miyawaki
  9. Kenta Sumiyama
  10. Kenta Terai
  11. Michiyuki Matsuda
(2022)
Functional visualization of NK cell-mediated killing of metastatic single tumor cells
eLife 11:e76269.
https://doi.org/10.7554/eLife.76269
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Abstract

Natural killer (NK) cells lyse invading tumor cells to limit metastatic growth in the lung, but how some cancers evade this host protective mechanism to establish a growing lesion is unknown. Here, we have combined ultra-sensitive bioluminescence imaging with intravital two-photon microscopy involving genetically encoded biosensors to examine this question. NK cells eliminated disseminated tumor cells from the lung within 24 hr of arrival, but not thereafter. Intravital dynamic imaging revealed that 50% of NK-tumor cell encounters lead to tumor cell death in the first 4 hr after tumor cell arrival, but after 24 hr of arrival, nearly 100% of the interactions result in the survival of the tumor cell. During this 24-hr period, the probability of ERK activation in NK cells upon encountering the tumor cells was decreased from 68% to 8%, which correlated with the loss of the activating ligand CD155/PVR/Necl5 from the tumor cell surface. Thus, by quantitatively visualizing, the NK-tumor cell interaction at the early stage of metastasis, we have revealed the crucial parameters of NK cell immune surveillance in the lung.

Editor's evaluation

This is an interesting study that significantly contributes to our understanding of the immunological mechanisms that limit cancer metastasis. Specifically, the authors make use of advanced imaging techniques to characterize the earliest responses of NK cells against tumor cells in cancer metastasis.

https://doi.org/10.7554/eLife.76269.sa0

Introduction

Natural killer (NK) cells are innate lymphoid cells that play critical roles in protecting against the development of tumor metastases (Chiossone et al., 2018). In human patients, a higher number of circulating or tumor-infiltrating NK cells is correlated with better patient outcomes (López-Soto et al., 2017). In immunocompetent mice, selective depletion of NK cells markedly increases the metastatic burden (Diefenbach et al., 2001; Smyth et al., 1999). Most of these previous studies relied on the number of macro-metastatic tumors as a single functional endpoint, preventing insight into the step(s) of the metastatic cascade at which NK cells play the most critical role. Metastasis involves the migration of a tumor cell or tumor cell cluster from the primary cancer site through the blood, lodging of the migrating cells in a micro-vessel, and the transmigration of the cell(s) into the tissue parenchyma, where they may either remain dormant or grow into a larger tumor mass (Gupta and Massagué, 2006). Given this sequence of events, it is unknown where NK cell attack on the malignant cells giving rise to a metastatic lesion takes place. Using a newly developed method of intravascular staining of immune cells (Anderson et al., 2014), it was shown that more than 90% of NK cells in the mouse lung are in the vasculature (Secklehner et al., 2019). In agreement with this finding, the major NK cell subset in the lung is similar to that in the peripheral blood (Hayakawa and Smyth, 2006; Marquardt et al., 2017). Meanwhile, it has also been proposed that NK cells in the normal lung are incompetent or hypofunctional (Marquardt et al., 2017; Robinson et al., 1984). Thus, it remains unclear how pulmonary NK cells are able to prevent tumor cells from colonization in the lung.

Inhibition of platelets and coagulation factors has long been associated with the suppression of lung metastasis (Brown, 1973; Gasic et al., 1968; Pearlstein et al., 1984). At least a part of the pro-metastatic effect of the coagulation cascade is attributed to inhibition of NK cells (Gorelik et al., 1984; Nieswandt et al., 1999; Palumbo et al., 2005; Sadallah et al., 2016). But other mechanisms such as enhanced adhesion of tumor cells (Nierodzik et al., 1992), formation of a favorable intravascular metastatic niche (Lucotti et al., 2019), or TGF-β1-mediated immune evasion (Metelli et al., 2020) have also been proposed. Therefore, a method to untangle the metastatic cascade in vivo is needed to quantitatively assess the effect of anticoagulants on each step and the possible relationship of this anti-metastatic action to the function of NK cells.

Intravital two-photon (2P) microscopy enables visualization of the interaction of immune cells with other immune cells or their targets (Cyster, 2010; Germain et al., 2012; Liew and Kubes, 2015). For example, the dynamic behaviors of NK cells have been demonstrated in the lymph nodes (Bajénoff et al., 2006; Beuneu et al., 2009; Mingozzi et al., 2016) and the tumor microenvironment (Barry et al., 2018; Deguine et al., 2010). Moreover, the development of genetically encoded biosensors for signaling molecules has paved the way to monitoring of cellular activation status in not only normal but also pathological tissues (Conway et al., 2017; Terai et al., 2019).

Here, we have combined bioluminescence whole-body imaging and intravital 2P microscopy to explore the behavior and functional competence of NK cells in an experimental lung metastasis model. Using an ultra-sensitive bioluminescence system, we followed the fate of intravenously injected tumor cells from 5 min to 10 days. The number of viable disseminated tumor cells in the lung decrease rapidly and reach a nadir within 12–24 hr in an NK cell-dependent manner. Intravital 2P microscopy demonstrates that a static tumor cell in a pulmonary capillary is contacted by a crawling NK cell approximately every 2 hr. Importantly, the probability of NK cell activation and subsequent elimination of the lodged tumor cell decreases rapidly after 24 hr of arrival in the lung capillary bed. We show that this evasion of NK cell surveillance is inversely correlated with thrombin-dependent shedding of CD155/PVR/Necl5 (hereafter simply Necl5), a ligand for the NK cell-activating receptor DNAM-1. This loss of surface activating ligand limits the signaling needed to invoke NK cytotoxicity, thus protecting the tumor cell and enabling the formation of a growing metastatic lesion. Anticoagulants promote tumor killing by NK cells by limiting this loss of activating ligand.

Results

NK cells eliminate disseminated tumor cells within 12–24 hr after the entry into the lung

Development of an extremely bright bioluminescence imaging system, AkaBLI (Iwano et al., 2018), enabled us to visualize the acute phase of lung metastasis and to explore the role of NK cells in the elimination of disseminated tumor cells. B16F10 melanoma cells were transduced with Akaluc luciferase, and the resulting cells, called B16-Akaluc cells hereafter, were injected intravenously into syngeneic C57BL/6 mice that had previously been injected with either an anti-asialo GM1 (αAGM1 hereafter) antibody or an isotype control antibody. The pretreatment with αAGM1 removed more than 97% of NK cells from the spleen and the lung (Figure 1—figure supplement 1A and B). Immediately after the intravenous injection of tumor cells, we administered AkaLumine luciferin intraperitoneally (i.p.) and started bioluminescence imaging under anesthesia (Figure 1A and Figure 1—video 1). A bioluminescence signal in the control mice was observed almost exclusively in the lung and decreased rapidly in the first 20 min, then gradually thereafter. In the αAGM1-treated mice, the bioluminescence signal dropped rapidly as observed in the control mice; however, the decrease was substantially reduced after 20 min as compared to control animals. Thus, in the initial phase (<180 min), there are at least two mechanisms that eliminate melanoma cells from the lung. The rapid elimination of melanoma cells (<20 min) may reflect flushing away by the blood flow or shear-stress-mediated cell death. The slow component of the elimination (>20 min) observed in the control mice is caused primarily by NK cells.

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NK cells eliminate a subset of metastatic tumor cells from the lung within 24 hr of arrival.

(A, B) B6 mice were pretreated with either control antibody or αAGM1. Representative merged images of the bright field and the bioluminescence images of mice intravenously injected with 5×105 B16-Akaluc cells are shown. (A) The substrate was i.p. administered immediately after injection of tumor cells. Image acquisition was started at 5 min after tumor injection. See also Figure 1—video 1. Bioluminescence intensity (BLI) is normalized to that at 5 min and plotted over time. Data are representative of two independent experiments with three mice per group and are shown as means ± SD. A dotted line represents 20 min. (B) Substrate was administered i.p. before each round of image acquisition. BLI is normalized to that at 1 hr. Data are representative of three independent experiments with 4–6 mice per group and shown as means ± SD. (C) B16-Akaluc cells were injected into the tail vein of mice that had been inoculated with B16F10 cells in the footpad 14 days before. BLI was quantified at the indicated time and normalized to that at 1 hr after injection of the B16-Akaluc cells. Data are representative of two independent experiments with three mice per group and are represented as means ± SD. (D) Nude mice were pretreated with either control antibody or αAGM1. 4T1-Akaluc cells were injected into the tail vein. BLI was quantified at the indicated time and normalized to that at 1 hr after injection of the tumor cells. Data are representative of two independent experiments with four mice per group and are represented as means ± SD. (E) BALB/c mice were pretreated with either control antibody or αAGM1. Shown are representative merged images of the bright field and the bioluminescence images of mice subcutaneously injected with 5×105 4T1-Akaluc cells into footpad. An arrow and asterisks depict a lung metastasis and primary tumors, respectively. Lung metastasis incidence of control antibody- (n=9) or αAGM1- (n=8) treated mice. (F, G) Identical to (E) except that mice are nude mice and the implanted cell number is 1×104. (F) BLI of primary tumor. Data are representative of two independent experiments with three mice per group and are represented as means ± SD. (G) Lung metastasis incidence of control antibody- (n=11) or αAGM1- (n=18) treated mice. NK, natural killer.

To explore the NK cell-mediated elimination of tumor cells after the early rapid phase decline (1 hr to 8 days), we administered luciferin immediately before each round of imaging (Figure 1B). The bioluminescence signals were normalized to that at 1 hr after B16-Akaluc injection in each mouse. In the control mice, the bioluminescence signal of melanoma cells reached a nadir 24 hr after tumor cell injection and increased thereafter, indicating proliferation of melanoma cells. On the other hand, in the αAGM1-treated mice, the bioluminescence signal decreased very little after 4 hr and started increasing after 12 hr. Importantly, after 24 hr, we did not observe any significant difference in the relative increase of the bioluminescence signal between the control and αAGM1-treated mice. In both mice, the doubling time of melanoma cells is approximately 1 day, implying that NK cells eliminate disseminated melanoma cells primarily in the acute phase (<24 hr) of lung metastasis. In tumor burden mice, the lung microenvironment is often reprogrammed in favor of metastasis (Altorki et al., 2019). To test this possibility, B16F10 melanoma cells were inoculated into the footpad 2 weeks prior to the intravenous injection of the B16-Akaluc cells (Figure 1C). In this model, B16F10 melanoma cells continue to grow at the footpad until the day of B16-Akaluc cell injection. αAGM1 treatment hampered the rapid decrease of the bioluminescence signal, suggesting that NK cell-mediated elimination of metastatic melanoma cells operates in the melanoma-burdened mice as well.

We extended this approach to other syngeneic mouse tumor cell lines: BrafV600E melanoma cells (Dhomen et al., 2009), MC-38 colon adenocarcinoma cells (Rosenberg et al., 1986), and BALB/c mice-derived 4T1 breast cancer cells (hereinafter called 4T1-Akaluk). The rapid decrease of bioluminescence signals was markedly alleviated by αAGM1, supporting the critical role of NK cells in the acute phase (Figure 1—figure supplement 2A–C). It has been reported that the αAGM1 reacts with basophils (Nishikado et al., 2011). Therefore, we repeated the experiment using an αCD200R3 basophil-depleting antibody (Ba103). The basophil depletion did not affect the elimination of melanoma cells (Figure 1—figure supplement 3A and B). Similarly, the roles of circulating monocytes and neutrophils were examined with clodronate liposome and αLy-6G neutrophil antibody, respectively. Neither treatment mitigated the melanoma elimination within 24 hr of injection (Figure 1—figure supplement 3C–F). Although the effect of these reagents to eliminate monocytes and neutrophils was not complete, these data suggest the involvement of monocytes and neutrophils in the rejection of melanoma cells in the acute phase.

The effect of T cell immunity on tumor elimination was examined by using Foxn1nu/nu mice (hereinafter called nude mice). 4T1-Akaluc cells were injected into nude mice (Figure 1D). 4T1-Akaluc cells were eliminated in mice as efficiently as in wild-type (WT) mice in an NK cell-dependent manner, indicating that under these conditions, T cell immunity does not contribute to tumor cell reduction in the acute phase of rejection (<24 hr). To further explore the NK cell-mediated tumor cell elimination in a spontaneous metastasis model, 4T1-Akaluc cells were inoculated into the footpad of WT and nude mice (Figure 1E–G). The αAGM1 treatment did not affect the growth of the primary tumor, but suppressed lung metastasis (Figure 1E and G). These results indicate the critical role of NK cells in the elimination of disseminated tumor cells. The experiment with nude mice also excluded the involvement of NKT and γδ T cells, with which αAGM1 reacts (Trambley et al., 1999). Of note, ILC1 cells also react with αAGM1. But, ILC1 is known to promote lung metastasis of B16F10 cells (Gao et al., 2017), suggesting that the effect of αAGM1 is primarily caused by the depletion of NK cells.

NK cell dynamic behavior in pulmonary capillaries

To better understand how NK cells mediate rapid elimination of metastatic tumor cells, we examined their topographic distribution and dynamics in the lung. We first assessed the localization of NK cells by intravascular staining with αCD45 antibody (Anderson et al., 2014), followed by flow cytometry with αCD45, αCD3, and αNCR1 antibodies (Figure 2—figure supplement 1). Consistent with previous reports (Gasteiger et al., 2015; Secklehner et al., 2019), more than 95% of pulmonary NK cells (CD45+, CD3−, and NCR1+) were found in the vasculature, compared to 20% of bone marrow NK cells. To study the dynamics of NK cell-mediated immune surveillance in the lung, we developed a reporter line, NK-tdTomato mice, whose NK cells, or more specifically, NCR1+ cells (Narni-Mancinelli et al., 2011), express the fluorescent protein tdTomato. Next, we employed in vivo pulmonary imaging by 2P microscopy to observe NK cells in situ for up to 12 hr (Figure 2A). In agreement with the flow cytometric data, most NK cells were found within the capillaries (Figure 2B). NK cells flowing in the capillaries stalled on endothelial cells, crawled a short distance, and jumped back into the flow (Figure 2C and Figure 2—video 1). A histogram of the crawling time exhibited exponential decay with a median of 2.5 min (Figure 2D). NK cells are known to express at least two integrin-family proteins, LFA-1 (LFA-1α/CD18 and αLβ2) and Mac-1 (Mac-1/CD18 and αMβ2) (Wang et al., 2012). Intravenous injection of the blocking antibody against LFA-1α (αLFA-1α) resulted in a reduction of NK cells on the pulmonary endothelial cells (Figure 2E). To extend this observation, we counted the number of NK cells on the endothelial cells in the presence or absence of αLFA-1α. As expected, αLFA-1α, but not αMac-1, markedly reduced the number of NK cells on the pulmonary endothelial cells (Figure 2F), indicating that the adhesion of NK cells to the pulmonary endothelial cells is mediated at least partially by LFA-1.

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NK cells patrol pulmonary capillaries in a stall-crawl-jump manner.

(A) A schematic of the intravital imaging system for the lung. The left lobe of the lung was exposed by 5th or 6th intercostal thoracotomy using custom-made retractors and fixed to the objective by a vacuum‐stabilized imaging window. (B) (Left) A micrograph of the lung of an NK-tdTomato mouse, in which NK cells express tdTomato (magenta). Lectin (green) was injected intravenously to stain endothelial cells. (Right) A magnified image of the boxed region in the left panel. (C) A representative time-lapse image of NK cells (magenta). The track of an NK cell is shown with a cyan dotted line and white arrowheads at both ends. White and yellow dotted circles show the positions of stall and jump, respectively. See also Figure 2—video 1. (D) Distribution of the crawling duration times in a 0.25-mm2 field of view (FOV). Data are pooled from two independent experiments (n=583). (E, F) B6 mice expressing tdTomato in NK cells (magenta) were observed by 2P microscopy. During time-lapse imaging with a 30-s interval, 100 µg of αLFA-1α, αMac-1, or isotype control antibody was intravenously injected. The number of NK cells in the 0.25-mm2 FOV was counted 0–10 min before and 30 min after antibody injection. The percentage of NK cells after versus before antibody injection is shown in (F). Data were pooled from three independent experiments and represented as means ± SD. n=3 mice for each group. 2P, two-photon; NK, natural killer.

Intra-pulmonary NK cell patrolling and tumor interaction dynamics

To understand better the kinetics of NK cell migration within pulmonary vessels and their interactions with lodged tumor cells, we examined the three-dimensional trajectory of the crawling NK cells in the presence and absence of B16F10 cells (Figure 3A–C). In this experiment, we used B16-SCAT3 cells, which expressed the Förster resonance energy transfer (FRET)-based caspase-3 biosensor SCAT3 (Takemoto et al., 2003). The ratio of NK cells versus tumor cells in the field of view (FOV) was set approximately 1:1. We compared the mean square displacement (MSD) of NK cells in the presence versus absence of tumor cells (Figure 3D). Curves fitted with the measured data represent α<1 regardless of the presence of tumor cells, α=0.56 in the presence and α=0.53 in the absence, indicating that the migration mode of NK cells can be classified as sub-diffusive. This is probably because the migration of NK cells is limited to the pulmonary vascular structure. MSD analysis also shows that the displacement from the original position is smaller in the presence than in the absence of tumor cells. This observation is consistent with our present finding that the mean instantaneous speed of the crawling NK cells was significantly decelerated in the presence of tumor cells, from 7.8 to 4.8 μm/min (Figure 3E). In accordance with this observation, the median duration time of crawling was markedly increased in the presence of tumor cells, from 5 to 30 min (Figure 3F). Notably, these data exclude regions in which the tumor cells would physically block NK movement in the capillary, suggesting that the dissemination of tumor cells causes global activation of pulmonary endothelial cells, and thereby causes slower crawling of NK cells. Taking advantage of these quantitative imaging data, we summarized parameters regarding the dynamics of pulmonary NK cells (Table 1). The parameters on flowing NK cells were deduced from the NK cell count in blood and the flow rate in pulmonary capillaries. In short, a tumor cell lodged in a pulmonary capillary will be contacted by the flowing and crawling NK cells roughly every 10 min and every 2 hr, respectively.

Figure 3
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NK cells patrol capillaries deliberately in the presence of melanoma.

NK-tdTomato mice were injected with 1.5×106 B16-SCAT3 cells and observed under a 2P microscope for 2 hr from 6 hr after injection. NK-tdTomato mice without any treatment were used as the control. SHG stands for second-harmonic generation. (A) A micrograph of the lung of an NK-tdTomato mouse. B16-SCAT3 cells, green; NK cells, magenta. (B) The average number of NK cells and tumor cells in each FOV at 10–35 µm from the pleura 10 min after intravenous injection of B16F10 cells (n=9). The red lines represent the mean. (C) Trajectories of crawling NK cells in the presence (left) or absence (right) of B16F10 cells. For 3D tracking, images of a 0.25-mm2 FOV and 25 µm thickness at 10–35 µm from the pleura were acquired every 30 s for 120 min. Shown here are the trajectories of NK cells projected onto the XY plane. Each track is shown in pseudo-color based on track duration. Data are at least from two independent experiments for each condition. n=1127 cells in the absence and n=718 cells in the presence of tumor cells. (D–F) Shown are mean squared displacement (MSD) (D), instantaneous speed (E), and track duration (F). The statistical differences between the two experimental groups were assessed by Mann–Whitney U-test. 2P, two-photon; FOV, field of view; NK, natural killer.

Table 1
Dynamics of NK cell killing of melanoma cells in the lung.
SymbolsParametersValuesUnitsReferences, equations, and comments
Histological and physiological parameters from published papers
BvBlood volume1.7E−6m3Table II (Davies and Morris, 1993)
LvLung volume3.7E−07m3Figure 2A for Week 8 mice (Gomes et al., 2019)
COCardiac output2.0E−05m3/minAbstract (Janssen et al., 2002)
Cp_lTotal lung capillary length1.1E+03mResult section (Knust et al., 2009)
Parameters determined experimentally
FOVField of view2.5E+07m20.5×0.5 mm2
Plt_speedPlatelet speed0.0570.95m/min mm/sDetermined as described previously (Sano et al., 2016).
Cp_rCapillary radius3.4E−06mMeasured on the images of Figure 2
NK_dNK cell diameter1.0E−5mMeasured on the images of Figure 2
NK_blNK cell count in blood5.1E+10cells/m3Determined for C57BL/6 mice of 8–12 weeks old.
NK_FOVNK cell number in a field of view16cells/FOVMeasured on the images of Figure 4
NK_speedNK crawling speed on capillaries4.8E−06m/minDetermined with time-lapse images of Figure 4
NK_hit_obsObserved NK cell hit probability8.0E−3cells/minDetermined with time-lapse images of Figure 4
NK_killNK cell killing probability0.5Determined with time-lapse images of Figure 4.
Ml_hl_BLIMelanoma half-life based on BLI data146minFrom bioluminescence images of Figure 1 at 4 hr.
Calculated parameters
Cp_frCapillary flow rate1.60E−12m3/minPlt_speed*π*Cp_r2
NK_wblWhole blood NK cells8.7E+04cellsNK_bl*Bv
NK_densityNK cell density in lung6.4E+12cells/m3NK_FOV/FOV/NK_d
NK_lungTotal NK cell in lung2.4E+06cellsNK_density*Lv
NK_inNK cell influx to lung1.0E+06cells/minCO*NK_bl
NK_outNK cell decay constant0.42/minNK_in/NK_lung
NK_hlNK cell half-life in the lung1.6minln2/NK_out
NK_frNK cell flow rate per capillary0.116.6cells/min cells/hrNK_bl*Cp_fr
NK_dcpNK cell density on capillary2.1E+03cells/mNK_lung/Cp_l
NK_hit_crCrawling NK cell hit probability0.0100.6cells/min cells/hrNK_dcp*NK_speed
Ml_t_2P_obsMelanoma decay constant calculated by2P imaging4.0E−03/minNK_kill*NK_hit_obs
Ml_hl_2P_obsMelanoma half-life based on 2P imaging data173minln2/Ml_t_2P_obs
Ml_t_2P_crspMelanoma decay constant based on crawling speed5.1E−03/minNK_kill*NK_hit_cr
Ml_hl_2P_crspMelanoma half-life based on crawling speed137minln2/Ml_t_2P_crsp

  1. Basic parameters: Macroscopic and histological data were based on previous papers (Gomes et al., 2019; Janssen et al., 2002; Knust et al., 2009). The speed of platelets in the lung capillaries (Plt_speed) was determined as described previously (Sano et al., 2016). The speed of platelets in the pulmonary capillaries was roughly one-third of the speed of platelets in the arteriole of mouse bladder, 3.1 mm/s (0.186 m/min) (Sano et al., 2016). The capillary radius, diameter of NK cells, and number of NK cells in a field of view were determined on at least three images. Plt_speed and Cp_r were used to calculate the capillary flow rate (Cp_fr). To determine the total number of NK cells in the blood, 50 µL of blood was collected from the right ventricle of 8- to 12-week-old C57BL/6 mice, lysed in ACK buffer (155 mM/L NH4Cl, 10 mM/L KHCO3, and 0.1 mM/L EDTA), and analyzed by flow cytometry. The CD3− NK1.1+ cells were counted as NK cells. This number of NK cells is two- to threefold larger than that reported previously by using C57BL/6J mice (Banh et al., 2012). The mean crawling speed on the endothelial cells is described in the text related to Figure 3E. The probability of an NK cell hitting a tumor cell was determined by a MATLAB script (Main_191017.m). The probability of an NK cell killing a tumor cell was 0.5, based on the probability of induction of calcium influx in the target B16 melanoma cells (Figure 4H).

  2. Total number of lung NK cells: The total number of NK cells residing in the lung (NK_lung) was estimated from the mean NK cell density (NK_density) and total lung volume (Lv). The diameter of an NK cell (NK_d) was used as the thickness of the image plane. The number of total NK cells, 2.4 million, is markedly larger than the previous values, which ranged from 0.2 to 1 million (Bi et al., 2017; Grégoire et al., 2007; Yan et al., 2014). In previous studies, the whole lungs were lysed to count the blood cell number. It is possible that the recovery rate might have been low due to insufficient tissue lysis. As described in the main text, we observed comparable numbers of tumor cells and NK cells in each FOV, when 1.5×106 B16-SCAT cells were injected into NK-tdTomato mice, supporting the fidelity of the number of total NK cells determined in this study.

  3. Dynamics of NK cells: Most of the pulmonary NK cells are within the vasculature (Figure 1—figure supplement 3), and the number of pulmonary NK cells overwhelms that of NK cells in the blood. Thus, the total number of lung NK cells can be used as the total number of NK cells in the lung vasculature. NK cell influx into the lung (NK_in) is obtained from cardiac output (CO) and NK cell count in the blood (NK_bl). If all NK cells stay in the lung with equal probability, the apparent transit time in the lung, or NK cell half-life in the lung, is calculated as 1.6 min from NK_in and NK_lung. This value is markedly smaller than the tracking duration period observed in Figures 3 and 4, indicating that the major population of NK cells in the blood go through the lung without adhesion to the endothelial cells. By using the capillary flow rate (Cp_fr) and NK cell count (NK_bl), the NK cell flow rate per capillary (NK_fr) is determined as 0.11 cells/min. Meanwhile, from the total length of capillaries (Cp_l) and the number of NK cells (NK_lung), NK cell density on the capillary (NK_dcp) is determined as 2.1 cells/mm. From NK_dcp and the crawling speed of NK cells, the probability of a tumor cell being hit by crawling NK cells (NK_hit_cr) becomes 0.010 cells/min. This value is approximately one-tenth of the flow rate of NK cells (NK_fr).

  4. Dynamics of disseminated melanoma cells: The BLI signals from 1 to 12 hr (Figure 1B) were fitted with MATLAB using the following equation: BLI=t-1.45t,hour .

  5. With this fitting, the decay rate decreases with time. Because we characterized the NK cell interaction with tumor cells between 4 and 8 hr after tumor cell injection, we determined the half-life of B16F-Akaluc cells from 4 hr (Ml_hl_BLI) and obtained 146 min. Meanwhile, from the probability of an NK cell hitting a tumor cell (NK_hit_obs) and the probability of an NK cell killing a tumor cell (NK_kill), the half-life of tumor cells (Ml_hl_2P_obs) becomes 173 min. If we adopt the probability of a tumor cell hit based on the crawling speed of NK cells, the expected half-life of tumor cells (Ml_hl_2P_crsp) becomes 137 min. Considering the precision of parameters obtained from in vivo imaging data, we believe that the half-life of melanoma cells estimated from the 2P microscopy reasonably matched the half-life of melanoma cells determined by BLI.

Necl5 and Nectin2 on tumor cells stimulate NK cell signaling leading to tumor cell killing

During serial killing of tumor cells by NK cells, perforin/GrzB initially plays a major role, followed by Fas-mediated killing (Prager et al., 2019). Therefore, we used two biosensors to detect NK cell-mediated killing in vivo: SCAT-3 for caspase activation by any pathway and GCaMP-6s for specific detection of the perforin/GrzB-mediated membrane damage. For the typical B16-SCAT3 cells, caspase-3 was activated 16 min after an NK cell came into contact with the tumor cell (Figure 4A and B and Figure 4—video 1). The caspase-3 activation was observed in 18% of contact events within a median of 26 min after the contact (Figure 4C and D). To examine the possible cause of this limited extent of measurable cell death after contact with an NK cell, we studied Ca2+ influx in tumor cells, which is known to herald apoptosis (Keefe et al., 2005), by using two Ca2+ sensors, GCaMP6s (Chen et al., 2013) and R-GECO1 (Zhao et al., 2011). In preliminary in vitro experiments, the B16F10 cells expressing R-GECO1 (B16-R-GECO) were co-cultured with NK cells that had been activated by IL-2 in vitro. Typically, Ca2+ influx was observed within a few min after contact (Figure 4—figure supplement 1A and B). A surge of Ca2+ influx was observed only in cells that were doomed to die (Figure 4—figure supplement 1C and Figure 4—video 2); 98% of cells that exhibited Ca2+ influx died by apoptosis with blebbing (Figure S5D). With these in vitro data in hand, we used the surge of Ca2+ influx as the surrogate marker for apoptosis of metastatic melanoma cells in vivo. In a typical example (Figure 4E and F and Figure 4—video 3), when an NK cell contacted a B16F10 cell expressing GCaMP6s (B16-GCaMP), Ca2+ influx was induced within 3 min. The Ca2+ influx was observed with a median lag of 6 min (Figure 4G) in 47% of contact events (Figure 4H). These data suggest that the reason why NK cells failed to induce caspase-3 activation in four-fifths of the tumor cells may be due to the limitation of observation period after the delivery of the lethal hit. In addition, the half-life of B16F10 cells based on the probability of an NK cell killing and crawling speed is 137 min whereas the one calculated based on the bioluminescence intensity (BLI) is 146 min (Table 1), suggesting that Ca2+ influx well correlates with BLI. It is reported that DNAM-1 on NK cells contributes to the elimination of B16F10 melanoma cells (Gilfillan et al., 2008). Therefore, to connect these data on tumor cell death with NK cell activation, we used B16F10 cells deficient in expression of CD155/PVR/Necl5 and CD112/Nectin2 and (Necl5 and Nectin2, hereafter), the ligands for the activating receptor DNAM-1 on NK cells (Chan et al., 2010). As anticipated, tumor Ca2+ influx was almost completely abolished in the Necl5−/− Nectin2−/− B16F10 cells (Figure 4H), suggesting that damage to tumor cells is dependent on the engagement of Necl5 and/or Nectin2 on melanoma cells.

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Intravital 2P imaging with biosensors visualizes apoptosis and calcium influx of tumor cells induced by crawling, but not flowing, NK cells.

(A) A representative time-lapse image of a lung of an NK-tdTomato mouse after B16-SCAT3 cell injection. An NK cell and B16-SCAT3 cells are depicted in magenta and green, respectively (top). Bottom, the CFP/FRET ratio in B16-SCAT3 cells is shown in the intensity-modulated display (IMD) mode and an NK cell is shown in white. See also Figure 4—video 1. (B) Quantification of the CFP/FRET ratio in a B16-SCAT3 cell in (A). (C) The percentage of NK cell-tumor cell contacts with or without caspase activation. Data were pooled from three independent experiments. (D) Time intervals between NK cell contact and caspase three activation in B16-SCAT3 cells. Data are pooled from three independent experiments. (E) A representative time-lapse image of a lung of NK-tdTomato mice after B16-GCaMP cell injection. An NK cell and B16-GCaMP cell are depicted in magenta and green, respectively (top). Bottom, GCaMP6s intensity in a B16-GCaMP cell is displayed in pseudo-color and an NK cell is shown in white. See also Figure 4—video 3. (F) Quantification of GCaMP6s intensity shown in (E). (G) Time intervals between NK cell contact and Ca2+ influx in B16-GCaMP cells. Data were pooled from four independent experiments. Red lines represent the median. (H) Comparison of the number of NK cell contacts that were followed by Ca2+ influx between the WT and Necl5−/− Nectin2−/−. Data were pooled from four (WT) and two (Necl5−/− Nectin2−/−) independent experiments. (I) In seven independent experiments, 40 contact events with calcium influx were observed and classified into those caused by crawling or flowing NK cells. (J) αLFA-1α or isotype control antibody was intravenously administered 2 hr before injection of 5×105 B16-Akaluc cells. The bioluminescence signals are normalized to those of 1 hr. Data are representative of two independent experiments with 3–4 mice per group and presented as means ± SD. (K) Representative macroscopic images of the metastasis to the lung and number of metastatic nodules per lung are shown. Red lines represent the median. Data were pooled from two independent experiments. Control, n=7; αLFA-1α, n=8. 2P, two-photon; NK, natural killer.

With these data in hand, we could return to the question of whether flowing or crawling NK cells are responsible for tumor cell death. Crawling NK cells accounted for 77% of Ca2+ influx events in the melanoma cells (Figure 4I). To reveal the impact of the crawling NK cells, αLFA-1α was used to inhibit NK cell attachment to the pulmonary capillaries. This markedly attenuated the melanoma elimination not only within 24 hr, but also after 10 days (Figure 4J and K). Our finding suggests that LFA-1 is required for the crawling of NK cells on the endothelial cells, and, thereby, for the immune surveillance against metastatic tumor cells. B16F10 cells do not express the LFA-1 ligands, ICAM-1 and ICAM-2 (Figure 4—figure supplement 2), arguing against the possibility that αLFA-1α directly impairs the association of NK cells with B16F10 cells, a conclusion also consistent with a previous study that demonstrated that LFA-1 deficiency in NK cells did not abrogate the in vitro killing capacity against B16F10 cells (Zhang et al., 2015).

Tumor-mediated stimulation of NK cells declines after several hours of pulmonary residence

To track tumor cell induction of NK cell activation, a key step in the killing process, we took advantage of evidence that engagement of LFA-1 or DNAM-1 with their ligands results in the activation of extracellular signal-regulated kinase (ERK) (Perez et al., 2003; Zhang et al., 2015). We isolated NK cells from transgenic mice expressing a FRET-based ERK biosensor (Komatsu et al., 2018), and co-cultured them with B16F10 cells in vitro. Quantification of ERK activity in each NK cell during contact with the tumor cells demonstrated a positive correlation between ERK activation in NK cells and apoptosis in tumor cells (Figure 5—figure supplement 1A). Apoptosis was induced in 47% of tumor cells that were in contact with the ERK-activated NK cells (Figure 5—figure supplement 1B). On the other hand, apoptosis was never observed in the tumor cells in contact with the NK cells that failed to exhibit ERK activation. In agreement with this observation, an inhibitor for MAPK/ERK kinase PD0325901, called MEKi hereafter, suppressed NK cell-mediated apoptosis (Figure 5—figure supplement 1C). When NK cells were sorted into DNAM-1+ and DNAM-1−, ERK was activated more potently in DNAM-1+ NK cells than in DNAM-1− NK cells (Figure 5—figure supplement 1D). In line with this observation, ERK was not activated in NK cells when B16F10 cells deficient from DNAM-1 ligands were used (Figure 5—figure supplement 1E and F). Previously, Du et al., 2018 reported that IL2-stimulated NK cells poorly recognize Necl5 and Nectin2-deficient B16F10 cells in vitro (Du et al., 2018). We confirmed this observation with three independent clones of Necl5−/− Nectin2−/− B16F10 cell (Figure 5—figure supplement 1G). These data support the critical role of DNAM-1 in ERK activation and induction of cytotoxicity at least in vitro.

The link between ERK activation and elimination of metastatic tumor cells was examined in vivo using bioluminescence imaging. At 1 hr before and 8 hr after the injection of B16-Akaluc cells, MEKi or solvent was administered i.p. into mice. MEKi significantly attenuated the rapid decrease of the injected tumor cell number within 24 hr (Figure 5A) and the number of lung colonies of MEKi-treated mice was significantly greater than in control mice (Figure 5B). At the same time, we observed that MEKi had no additive effect in αAGM1-treated mice in the early (<24 hr) time courses (Figure 5A). Although interpretation is limited by the action of the soluble inhibitor on cells other than NK cells, these additional data are consistent with our imaging data and the idea that activated NK cell contributes to the elimination of disseminated tumor cells and that ERK activation can be used as a marker for activated NK cells.

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Contact-induced ERK activation in NK cells is a necessary event in induction of apoptosis in tumor cells in the first 4 hr, but not after 24 hr.

(A) B6 mice were pretreated with either control antibody or αAGM1 and intravenously injected with 5×105 B16-Akaluc cells. At 1 hr before and 8 hr after injection, a MEK inhibitor (MEKi) or DMSO was administered i.p. Time courses of the signals, which are normalized to those at 1 hr after tumor injection for each mouse. Data are representative of two independent experiments and shown as means ± SD. n.s., not significant. (B) Macroscopic images were acquired at day 14. The number of metastatic colonies is shown. Control, n=5; MEKi, n=7. (C) A time-lapse image of the lung of an NK-ERK mouse expressing the FRET biosensor for ERK. The mouse was intravenously injected with B16-GCaMP cells. Top, FRET/CFP ratio of an NK cell (yellow arrowhead) is shown in IMD mode. A B16-GCaMP cell is shown in white. Bottom, GCaMP6s intensity is displayed in pseudo-color. The NK cell is shown in white. (D) Time course of the FRET/CFP ratio in the NK cell and CaMP6s intensity in the B16-GCaMP cell. (E) Activation probability of ERK in the NK cells upon target cell contact at 0–4 hr or 24 hr after tumor injection. Data were pooled from three independent experiments. (F) The probability of NK cells that exhibited ERK activation with or without induction of Ca2+ influx in the target tumor cells at 0–4 hr or 24 hr after tumor injection. Data were pooled from three independent experiments. (G) B16-Akaluc cells were injected into the tail vein of mice that had been injected PBS or B16F10 cells into tail vein 24 hr before. BLI was quantified at the indicated time and normalized to that at 1 hr after injection of B16-Akaluc cells. Data are representative of two independent experiments with three mice per group and are represented as means ± SD. BLI, bioluminescence intensity; FRET, Förster resonance energy transfer; IMD, intensity-modulated display; NK, natural killer; PBS, phosphate-buffered saline.

With these data in hand, we next proceeded to visualize ERK activation in vivo. For this, we developed reporter mice whose NK cells express the FRET biosensor for ERK, hereinafter called NK-ERK mice. Intravenous injection of B16-GCaMP cells into NK-ERK mice allowed for simultaneous observation of ERK activity in NK cells and Ca2+ influx in melanoma cells. In a representative example, ERK was activated 2.5 min after an NK cell’s contact with a melanoma cell (Figure 5C, upper panel; Figure 5D, magenta), followed by Ca2+ influx in the melanoma cells at 5.5 min and cell death at 10 min (Figure 5C, lower panel; Figure 5D, green). ERK activation, defined by a more than 30% increase in the FRET/CFP ratio, was observed within 3 min in 60 NK cells during 88 contact events (Figure 5—figure supplement 2A; Figure 5E). Ca2+ influx was observed at a median of 4 min in 43 of the 60 tumor cells that came into contact with the NK cell having ERK activation (Figure 5—figure supplement 2B; Figure 5F). We did not observe Ca2+ influx in 28 tumor cells that were touched by the NK cells that failed to show evidence of ERK activation. This result supports the notion that ERK activation in NK cells contributes to the induction of apoptosis in the target tumor cells. Importantly, 24 hr after injection, the probability of ERK activation and Ca2+ influx was markedly decreased, indicating NK cells lose the capacity to activate in response to capillary-lodged tumor cells (Figure 5E and F).

These results imply that NK cells in the lung are exhausted in 24 hr. Our quantitative data shows that 2.4 million NK cells in the lung outnumber 0.5 million melanoma cells injected into circulation (Table 1). Therefore, if NK cell exhaustion could happen, it is not caused by the killing of tumor cells, but by an indirect mechanism such as cytokine-induced suppression or endothelial cell-mediated inactivation. To understand the basis for this loss of NK cell activity by 24 hr after tumor arrival in the lung, B16F10 melanoma cells without Akaluc were injected 24 hr before the injection of B16-Akaluc cells (Figure 5G). We did not observe any effect of the pre-injected B16F10 cells on the time course of clearance of the B16-Akaluc cells, indicating that NK cells do not lose tumoricidal activity, but that over time, the tumor cells acquire the capacity to evade NK cell surveillance.

Thrombin-mediated shedding of Necl5 correlates evasion of NK cell surveillance

DNAM-1-mediated signaling contributes to tumoricidal activity of NK cells, leading us to reason that cell surface expression of the DNAM-1 ligands Necl5 and Nectin2 may diminish over this time period. Because the expression of Nectin2 was significantly less than that of Necl5 in B16F10 melanoma cells, we focused on Necl5. As anticipated, cell surface expression of Necl5 was markedly decreased in tumor cells isolated from the lungs 24 hr after injection (Figure 6A and B). To explore the basis for this change, we expressed a recombinant Necl5 fused extracellularly to the mScarlet fluorescent protein and intracellularly to the mNeonGreen fluorescent protein (Figure 6C). The ratio of extracellular mScarlet versus intracellular mNeonGreen was markedly reduced in 24 hr, indicating loss of extracellular domain, possibly by cleavage or shedding (Figure 6D and E). A clue to the mechanism of this Necl5 loss came from evidence that inhibition of serine proteases in the coagulation cascade has anti-tumor effects in rodent models and human patients (Francisco and Palumbo, 2019; Nierodzik and Karpatkin, 2006). Warfarin, an anti-vitamin K drug, potently accelerated the acute elimination of tumor cells (Figure 6F). Similarly, specific inhibitors of factor Xa and thrombin, edoxaban, and dabigatran etexilate, respectively, also promoted the elimination of tumor cells (Figure 6G and H). Notably, dabigatran etexilate did not have significant effect in αAGM1-treated mice (Figure 6H), indicating that the anti-metastatic effect is mediated by NK cells. In agreement with these functional results, thrombin cleaved off the extracellular domain of Necl5 from tumor cells in vitro (Figure 6I), and dabigatran etexilate suppressed the cleavage of mScarlet-tagged Necl5 in vivo (Figure 6I and J). Since dabigatran etexilate-treated mice often suffered from bleeding, we used edoxaban to address the long-term effect. The mice treated with edoxaban eliminated tumor cells almost completely, supporting the idea that the suppression of Necl5 cleavage promotes the elimination of disseminated tumor cells by NK cells (Figure 6—figure supplement 1). Several mechanisms have been proposed for coagulation cascade-mediated NK cell inhibition (Francisco and Palumbo, 2019), including that platelet-tumor aggregates physically protect tumor cells from NK cells (Cluxton et al., 2019; Nierodzik and Karpatkin, 2006). However, we rarely observed microthrombi around the disseminated tumor cells, even when a microthrombus was easily induced by laser ablation in the vicinity of the tumor cell (Figure 6—figure supplement 2 and Figure 6—video 1). Considering the role of platelets as the platform for coagulation factors, platelets may play a pro-metastatic role by promoting thrombin activation and thereby Necl5 shedding from the metastatic tumor cells.

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Shedding of Necl5 correlates evasion of NK cell surveillance.

(A, B) B16-Akaluc cells were injected into the tail vein and the expression level of Necl5 on survived tumor cells was analyzed at 24 hr after dissemination. The MFI of Necl5 in tumor cells injected 0 hr or 24 hr before is shown in (B). Red lines represent the median. Data were pooled from two independent experiments. (C) Schematic representation of the Necl5-ScNeo fusion protein. (D) The representative images of mScarlet/mNeonGreen ratio in the B16F10 cells expressing Necl5-ScNeo at 0.5 hr and 24 hr after injection are shown in the IMD mode. The quantified mScarlet/mNeonGreen ratio in the transmembrane in indicated time point is shown in (E). Data were pooled from three animals. Mice were treated in their drinking water with 5 mg/L warfarin at least for 5 days and intravenously injected with 5×105 B16-Akaluc cells. The BLI at 24 hr, which normalized to those at 1 hr after tumor injection for each mouse are shown. Red lines represent the median. Data were pooled from two independent experiments. (G, H) Mice were intravenously injected with 5×105 B16-Akaluc cells. At 1 hr before and 12 hr after tumor injection, edoxaban, dabigatran etexilate, or vehicle was orally administered to mice. For NK cell depletion, mice were pretreated with either control antibody or αAGM1. The BLI at 24 hr, which normalized to those at 1 hr after tumor injection for each mouse is shown. Red lines represent the median. Data were pooled from two independent experiments. (I) Flow cytometric analysis of B16F10 cells treated with recombinant thrombin for 3 hr. Data are representative of two independent experiments with three wells per group and are represented as means ± SD. (J) Mice were orally administrated with dabigatran etexilate 1 hr before tumor injection and analyzed as in (D, E). Data were pooled from three animals. (K) Evasion of NK cell surveillance by shedding of Nec-l5. NK, natural killer.

Finally, we attempted to examine if the loss of Necl5 and Nectin2 on B16F10 cells cause NK cell evasion in vivo, as was the case in vitro (Figure 5—figure supplement 1G). Surprisingly, whereas we did not observe Ca2+ influx after the NK cell contact with the Necl5−/− Nectin2−/− B16F10 cell (Figure 4H), the Necl5−/− Nectin2−/− B16F10 cells expressing AkaLuc were eliminated as efficiently as the parent B16F10 cells under the bioluminescence imaging (Figure 6—figure supplement 3). This observation probably indicates that an alternative pathway(s) are also involved in the Necl5−/− Nectin2−/− B16F10 cell rejection by NK cells in vivo.

Discussion

Despite the established role of NK cells in the prevention of metastasis (López-Soto et al., 2017), the step(s) of the metastatic cascade at which NK cells eliminate disseminated tumor cells remain unknown. Here, we adopted the AkaBLI system, by which even a single Akaluc-expressing tumor cell could be detected in mice (Iwano et al., 2018), and followed the fate of intravenously injected tumor cells from 5 min to 10 days after the injection of tumor cells (Figure 1). In agreement with previous studies (Grundy et al., 2007; Hinuma et al., 1987), the number of tumor cells decreased rapidly in an NK cell-dependent manner. However, we noticed that as early as 24 hr after injection, tumor cells started to increase and formed macrometastatic nodules, irrespective of the presence or absence of NK cells. Our results demonstrate that the principal role of NK cells in the prevention of lung metastasis is to destroy tumor cells shortly after their arrival and lodging in the pulmonary vasculature, but not thereafter. Using intravital imaging, Headley et al., 2016 found that tumor microparticles are rapidly ingested by myeloid cells to evoke an immune response (Headley et al., 2016). However, depletion of myeloid lineage cells did not affect the development of metastasis in the models we employed (Figure 1—figure supplement 3), excluding a role of the myeloid cells in the clearance of disseminated tumor cells in the immediate-early phase. Patrolling behavior similar to that of NK cells has also been observed for intravascular monocytes in the skin (Auffray et al., 2007). Like NK cells, the crawling monocytes require LFA-1 for their crawling. However, again, depletion of monocytes did not prevent the rapid clearance of disseminated tumor cells (Figure 1—figure supplement 3). Thus, the rapid elimination of the disseminated tumor cells within 24 hr is dependent primarily on NK cells in our models.

The crawling NK cells induce pre-apoptotic calcium influx in approximately 50% of the tumor cells that they contact (Figures 4H and 6K), indicating that pulmonary NK cells can eliminate the disseminated tumor cells as efficiently as do chimeric antigen receptor (CAR) T cells (Cazaux et al., 2019). Our findings are superficially inconsistent with reports that lung NK cells exhibit highly differentiated and hypofunctional phenotypes in vitro (Hayakawa and Smyth, 2006; Marquardt et al., 2017; Robinson et al., 1984). This discrepancy probably arises from the fact that most of the tumor cells were killed by NK cells crawling on the pulmonary endothelial cells, but not by those flowing in the blood. NK cells adhere to the endothelial cells in an LFA-1-dependent manner (Figure 4J). Binding of LFA-1 to its ligand ICAM-1 induces reorganization of the actin cytoskeleton and polarization of NK cells, which is a prerequisite for subsequent redistribution of cytotoxic granules toward the bound targets (Mace et al., 2009). It is likely that LFA-1 engagement of ICAM on pulmonary endothelial cells contributes to the pre-activation status of NK cells. In this regard, the slow migration speed of NK cells in the presence of tumor cells may indicate the increased fraction of active NK cells (Figure 3).

In the B16F10 melanoma metastasis model, DNAM-1 expression in NK cells contributes to the rejection of tumor cells (Gilfillan et al., 2008). In agreement with a previous report (Zhang et al., 2015), we have shown that, upon target cell engagement, ERK is rapidly activated in DNAM-1+ NK cells, but not DNAM-1− NK cells (Figure 5—figure supplement 1D). Simultaneous in vivo visualization of ERK activity in NK cells and Ca2+ influx in tumor cells revealed highly efficient tumor cell killing by NK cells showing evidence of effective signaling based on ERK activation (Figure 5E and F). Only about 60% of lung NK cells express DNAM-1 (Tahara-Hanaoka et al., 2005). However, most of the tumor cells were killed by the NK cells crawling on the pulmonary endothelial cells, but not by those flowing in the blood. Because DNAM-1 serves as an adhesion molecule (Kim et al., 2017; Shibuya et al., 1996), the crawling NK cells may be biased to DNAM-1+ NK cells, consistent with the potent cytotoxic activity of the crawling cells.

The discrepancy of the effect of Necl5 and Nectin2 knockout between in vitro and in vivo reflects the complexity of the mechanism of activation and cytotoxicity of NK cells (Figure 5—figure supplement 1G and Figure 6—figure supplement 3). First, Gilfillan et al., 2008 observed that the number of lung metastasis was significantly increased in DNAM-1-deficient mice, but markedly less than mice injected with αAGM1, indicating that DNAM-1-Necl5 interaction is not the only mechanism of B16F10 rejection by NK cells (Gilfillan et al., 2008). Second, Chan et al., 2010 reported that lung metastasis of B16F10 cells was impaired in DNAM-1 deficient mice treated with cytokines; however, neither DNAM-1 deficiency nor anti-DNAM-1 did not exhibit significant effects on the lung metastasis in the absence of cytokine administration (Chan et al., 2010). Because we stimulated NK cells with IL2 only in vitro, our observation agrees with this report. Third, Li et al., 2018 reported that Necl5-deficient B16F10 cells form lung metastasis less efficiently than WT cells because Necl5 is critical for tumor cell migration and survival (Li et al., 2018). Therefore, the effect of reduced sensitivity to NK cells may be masked by the other effects of Necl5 and Nectin2 deficiency. Moreover, there are three receptors, DNAM-1, TIGIT, and CD96, that bind to Necl5 with different affinity, 119, 3.15, and 37.6 nM, respectively (Martinet and Smyth, 2015). Since the two inhibitory receptors, TIGIT and CD96, exhibit higher affinity than the activating receptor DNAM-1, thrombin-mediated reduction of Necl5 may strengthen the inhibitory signal. Finally, the discrepancy could also be explained by the previous reports that TIGIT+ NK cells can eliminate Necl5−/− cells in vivo by missing-self recognition due to the education via Necl5 on the host cells (He et al., 2017) and that the effect of education on degranulation does not last in cell culture with IL2 (Pugh et al., 2019). The elimination mechanism of Necl5 and Nectin2 knockout cells is suggested to be NK cell-dependent but Ca2+ influx-independent manners because we did not detect Ca2+ influx in Necl5 and Nectin2 knockout cells in vivo (Figures 4H and 6K).

Shedding of ligands for the activating receptors of NK cells has been documented for NKG2D (Raulet et al., 2013). The NKG2D ligands, MICA, MICB, and ULBP2 are cleaved by matrix metalloproteases (MMPs), leading to evasion of NK surveillance. It is also reported that platelets can promote the MMP-mediated shedding of the NKG2D ligands in vitro (Maurer et al., 2018). However, to the best of our knowledge, involvement of thrombin or factor Xa in the shedding of the ligands for activating receptors such as Necl5 has not been reported. Interestingly, Necl5 contributes to cell adhesion as does DNAM-1 (Takai et al., 2008). Therefore, Necl5 on tumor cells is a double-edge sword, which facilitates adhesion to the lung capillary but also invokes NK cell attack. To evade the NK cell surveillance, after anchoring to the capillaries, tumor cells are able to take advantage of the capacity of thrombin to strip Necl5 from the cell surface within 24 hr after adhesion (Figure 6J). This new understanding of how NK cell surveillance of tumor cells is regulated in the micro-circulation provides a rationale for the development of new ways to inhibit the growth of clinically significant lung metastases.

Materials and methods

Plasmids

Plasmids encoding R-GECO1, SCAT3, GCaMP6s, mScarlet were obtained from Takeharu Nagai (Zhao et al., 2011), Masayuki Miura (Takemoto et al., 2003), and Addgene (plasmid # 40753 for GCaMP6s; #85044 for mScarlet; Cambridge, MA), respectively. The cDNAs of mNeonGreen (Shaner et al., 2013) was synthesized with codon optimization by GeneArt (Thermo Fisher Scientific, Waltham, MA). A plasmid encoding tdTomato was obtained from Takara Bio (#632533; Kusatsu, Japan). pPBbsr2-Venus-Akaluc was described previously (Iwano et al., 2018). For the gene knockout, lentiCRISPR v2 vector (Addgene plasmid #52961) was used. Plasmids pCSIIhyg-R-GECO1 and pCSIIbsr-GCaMP6s, lentiviral vectors for R-GECO1 and GCaMP6s, respectively, were constructed by inserting cDNAs into pCSII-based lentiviral vectors (Miyoshi et al., 1998) with IRES-hyg (hygromycin B-resistance gene) or IRES-bsr (blasticidin S-resistance gene). psPAX2 (Addgene plasmid #12260) and pCMV-VSV-G-RSV-Rev (provided by Hiroyuki Miyoshi at RIKEN) were used for the lentivirus production. To generate pPBbsr-SCAT3-NES, cDNA coding the SCAT3 fused with the nuclear export signal (NES) (LQLPPLERLTLD) of the HIV-1 rev protein (Fischer et al., 1995) was subcloned into pPBbsr, a PiggyBac transposon vector with IRES-bsr (Yusa et al., 2009). To generate pPBbsr2-Necl5-ScNeo, cDNA coding the signal peptide of Necl5 (a.a. 1–28), mScarlet, Necl5 (a.a. 29–408), and mNeonGreen were PCR-amplified and assembled into pPBbsr2 vector by using In-Fusion system (Takara Bio USA, Inc, Mountain View, CA). pCMV-mPBase (obtained from the Wellcome Trust Sanger Institute) was co-transfected with pPB vector to establish stable cell lines. To generate pT2Aneo-tdTomato-CAAX, cDNA encoding tdTomato fused with the CAAX domain of the KRas protein (a.a. 170–189) was subcloned into pT2Aneo vector (obtained from Kawakami et al., 2004), a Tol2 transposon vector with IRES-neo (neomycin-resistance gene). To generate transgenic mice, pT2ADW-lox-mCherry-hyBRET-ERK-NLS was constructed by assembling cDNAs of hyBRET-ERK-NLS (Komatsu et al., 2018), mCherry, and the NES sequence of the HIV-1 rev protein into pT2ADW vector (Komatsu et al., 2018) by In-Fusion cloning (Takara Bio).

Reagents

PD0325901 (FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan) was applied as a MEK inhibitor. Warfarin, Lixianar (edoxaban), and Prazaxa (dabigatran etexilate) were obtained from Eisai Co., Ltd (Tokyo, Japan), Daiichi Sankyo Company, Limited (Tokyo, Japan), and Boehringer Ingelheim GmbH (Ingelheim, Germany), and used as a vitamin K inhibitor, factor Xa (FXa) inhibitor, and thrombin inhibitor, respectively. AkaLumine-HCl (TokeOni) was obtained from Kurogane Kasei Co., Ltd (Nagoya, Japan) or synthesized as previously described (Kuchimaru et al., 2016) and used as the substrate of Akaluc. Collagenase type IV and DNase I were obtained from Worthington Biochemicals (Lakewood, NJ) and Roche (Basel, Switzerland), respectively. A LIVE/DEAD Fixable Red Dead Cell Stain Kit (Thermo Fisher Scientific) or 7-AAD (BD Bioscience) was used to stain dead cells in flow cytometry. DyLight 488-labeled Lycopersicon esculentum lectin was purchased from Vector Laboratories (Burlingame, CA). Recombinant mouse protein C and factor Xa were obtained from R&D Systems, Inc (Minneapolis, MN). Recombinant mouse thrombin was obtained from antibodies-online GmbH (Aachen, Germany).

Antibodies

The following antibodies were used for staining: BV510 or FITC anti-CD45 (30-F11), APC-Cy7 anti-CD3 (145–2C11), PerCP-Cy5.5 anti-NK1.1 (PK136), APC or PE-Cy7 anti-DNAM-1 (10E5), PE anti-F4/80 (BM8), APC anti-CD11b (M1/70), PE anti-NCR1 (29A1.4), PE anti-Ly-6G (1A8), PE anti-c-Kit (2B8), APC anti-CD49b (DX5), PE-Cy7 anti-CD200R3 (Ba13), PE anti-ICAM-1 (YN1/1.7.4), Alexa 488 anti-ICAM-2 (3C4), PE-anti PVR/Necl5 (TX56) (all from BioLegend, San Diego, CA), recombinant mouse DNAM-1 Fc chimera protein (R&D Systems), and Alexa Fluor 647 goat anti-mouse IgG (H + L) cross-adsorbed secondary antibody (Thermo Fisher Scientific). The following antibodies were used for in vivo blocking experiments: anti-LFA-1α (M17/4), anti-Mac-1 (M1/70) (both from Bio X Cell, West Lebanon, NH), and Rat IgG2a isotype control antibody (RTK2758; BioLegend). The following antibodies or reagents were used for in vivo cell depletion: anti-asialo GM1 (FujiFilm Wako Pure Chemical Corporation, Osaka, Japan), Rabbit IgG isotype control (Thermo Fisher Scientific), anti-Ly6G (1A8; BioLegend), Rat IgG2a isotype control, anti-CD200R3 (Ba103; Hycult Biotech, Uden, the Netherlands), Rat IgG2b isotype control (RTK4530; BioLegend), clodronate liposomes (Hygieia Bioscience, Osaka, Japan), or control liposome (Hygieia Bioscience).

Tumor cells

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The melanoma cell line B16F10 was purchased from the Cell Resource Center for Biomedical Research (Sendai, Japan). The MC-38 mouse colon adenocarcinoma cell line was provided by Takeshi Setoyama and Tsutomu Chiba at Kyoto University. The BrafV600E melanoma cell line (Dhomen et al., 2009) was provided by Caetano Reis e Sousa at the Francis Crick Institute. 4T1 mammary tumor cells were purchased from ATCC (Manassas, VA) and maintained on a collagen-coated dish (AGC Techno Glass, Tokyo, Japan).

Cell culture

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All cell lines were cultured in complete RPMI medium (Thermo Fisher Scientific) containing 10% fetal bovine serum (FBS) (Sigma-Aldrich, St. Louis, MO), 1 mM sodium pyruvate (Thermo Fisher Scientific), 50 μM 2-mercaptoethanol (Nacalai Tesque), 1% GlutaMAX solution (Thermo Fisher Scientific), 1% MEM non-essential amino acids (Thermo Fisher Scientific), 10 mM HEPES solution (Thermo Fisher Scientific), 50 μM 2-mercaptoethanol (Nacalai Tesque), 100 units/ml penicillin, and 100 μg/ml streptomycin (Nacalai Tesque, Kyoto, Japan). Mycoplasma contamination is regularly checked using PlasmoTest mycoplasma detection kit (InvivoGen, San Diego, CA).

Establishment of stable cell lines

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To prepare the lentivirus, pCSIIhyg-R-GECO1 or pCSIIbsr-GCaMP6s was cotransfected with psPAX2 and pCMV-VSV-G-RSV-Rev into Lenti-X 293T cells (Clontech, Mountain View, CA) with Polyethylenimine ‘Max’ (Mw 40,000; Polysciences, Warrington, PA). Virus-containing media were harvested 48 hr after transfection, filtered, and used to infect B16F10 cells to yield B16-R-GECO cells and B16-GCaMP cells. For the transposon-mediated gene transfer, pPBbsr-SCAT3-NES, pPBbsr2-Venus-Akaluc, or pPBbsr2-Necl5-ScNeo was cotransfected with pCMV-mPBase into B16F10 cells by using Lipofectamin 3000 reagent (Thermo Fisher Scientific), yielding B16-SCAT3 cells, B16-Akaluc cells, and B16-Necl5-ScNeo cells, respectively. pT2Aneo-tdTomato-CAAX was cotransfected with pCS-TP into B16-GCaMP6 cells by using Lipofectamin 3,000 reagent, yielding B16-GCaMP-tdTomato-CAAX cells. pPBbsr2-Venus-Akaluc was cotransfected with pCMV-mPBase into BrafV600E melanoma cells, MC-38 cells, and 4T1 cells by using Lipofectamin 3000 reagent. Cells were selected with either 10 μg/ml blasticidin S (Calbiochem, San Diego, CA) or 100 μg/ml hygromycin B (FujiFilm Wako Pure Chemical Corporation).

CRISPR/Cas9-mediated establishment of KO cell lines

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For CRISPR/Cas9-mediated KO of tyrosinase (Tyr), Necl5, and Nectin2, single-guide RNAs (sgRNA) targeting the first or second exon were designed using the CRISPRdirect program (http://crispr.dbcls.jp/). For the establishment of double knockout cells, a puromycin-resistant gene in lentiCRISPR v2 vector was replaced with a bleomycin-resistant gene. The targeting sequences were as follows: Tyr, GGGTGGATGACCGTGAGTCC; Necl5, GCTGGTGCCCTACAATTCGAC; Nectin2, GACTGCGGCCCGGGCCATGGG. Annealed oligo DNAs for the sgRNAs were cloned into the lentiCRISPR v2 vector. The sgRNA/Cas9 cassettes were introduced into cells by lentiviral gene transfer. Infected cells were selected by 3.0 μg/ml puromycin (InvivoGen) or 100 µg/ml zeocin (Thermo Fisher Scientific). Cells deficient for Necl5 and Nectin2 were sorted by a FACS Aria IIu cell sorter and used without single-cell cloning. Tyr-KO cells were subjected to single-cell cloning and examined for the frame-shift mutation by nucleotide sequencing.

Mice

C57BL/6N (hereinafter called B6) mice, BALB/c mice, and nude mice were purchased from Shimizu Laboratory Supplies (Kyoto, Japan) and bred at the Institute of Laboratory Animals, Graduate School of Medicine, Kyoto University under specific-pathogen-free conditions. B6N-Tyrc-Brd/BrdCrCrl (hereinafter called B6 Albino) mice were obtained from Charles River Laboratories. Mice of either sex were used at the age of 6–18 weeks. B6.Cg-Gt(ROSA)26Sortm9(CAG-tdTomato)Hze/J mice (JAX 007909) were obtained from the Jackson Laboratory (Bar Harbor, ME). B6(Cg)-Ncr1tm1.1(icre)Viv/Orl mice (Narni-Mancinelli et al., 2011) (hereinafter called Ncr1iCre mice) were obtained from INFRAFRONTIER (Oberschleissheim, Germany). Transgenic mice expressing hyBRET-ERK-NLS have been described previously (Komatsu et al., 2018). B6.Cg-Gt(ROSA)26Sortm9(CAG-tdTomato)Hze/J mice were crossed with Ncr1iCre mice for NK cell-specific expression of tdTomato, resulting in Ncr1iCre/ B6.Cg-Gt(ROSA)26Sortm9(CAG-tdTomato)Hze/J mice (hereinafter called NK-tdTomato mice). Tg(lox-mCherry-hyBRET-ERK-NLS) mice were crossed with Ncr1iCre mice for NK cell-specific expression of hyBRET-ERK-NLS, resulting in Ncr1iCre/ Tg(lox-mCherry-hyBRET-ERK-NLS) mice (hereinafter called NK-ERK mice). Mice of either sex were used for experiments without specific randomization and blinding. We performed at least two independent experiments with at least three mice each for the condition of interest. For the imaging experiments, if we failed to see any fluorescence or bioluminescence signal, the mice were excluded from the analysis. The animal protocols were reviewed and approved by the Animal Care and Use Committee of Kyoto University Graduate School of Medicine (Approval no. 19090).

Generation of transgenic mice

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Transgenic mice were generated by Tol2-mediated gene transfer as previously described (Sumiyama et al., 2010). Briefly, fertilized eggs derived from B6 mice were microinjected with a mixture of Tol2 transposase mRNA and pT2ADW-lox-mCherry-hyBRET-ERK plasmid. The offspring mice, named Tg(lox-mCherry-hyBRET-ERK-NLS), were then backcrossed with B6 Albino mice for at least three generations. Newborn mice were illuminated with a green LED and inspected for red fluorescence through a red filter LED530-3WRF (Optocode, Tokyo).

In vivo cell depletion

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To deplete NK cells, mice were injected i.p. with 20 μg αAGM1 or rabbit IgG isotype control antibody on 1 and/or 2 days before tumor cell injection. In some experiments, the antibody administration was repeated on days 0 and 7 after tumor cell injection. To deplete basophils, 30 μg αCD200R3 (Ba103) or rat IgG2b isotype control antibody was injected i.p. at 1 day before tumor cell injection. To deplete neutrophils, 200 μg anti-Ly6G (1A8) or rat IgG2a isotype control was injected i.p. at 1 day before tumor cell injection. To deplete monocytes and macrophages, clodronate liposome (50 mg/kg) or control liposome was injected i.p. at 1 day before tumor cell injection. The efficiency of the depletion was assessed by flow cytometry.

In vivo blocking of integrins

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NK-tdTomato mice were injected i.v. with 100 μg of αLFA-1α, αMac-1, or Rat IgG2a antibody during image acquisition. To visualize the vascular structure, 50 μg of DyLight 488-labeled lectin was intravenously injected. The number of NK cells in the 0.25-mm2 FOV was counted 0–10 min before and 30 min after antibody injection. Image acquisition and analysis were carried out with MetaMorph software (Molecular Devices LLC, Sunnyvale, CA).

Staining of intravascular NK cells of the bone marrow and lung

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Mice were subjected to intravenous injection of the 3 μg αCD45 antibody 3 min before sacrifice. Bone marrow cells were harvested by flushing the femoral bone with 5 ml RPMI containing 10% FBS, 100 units/ml penicillin, and 100 μg/ml streptomycin. Red blood cells were removed by lysis with ACK lysing buffer and centrifugation at 500×g for 5 min at 4℃. A single-cell suspension of the lung cells was generated by mincing the resected lungs with scissors and incubating the minced tissue in RPMI containing 200 U/ml collagenase type IV and 5 U/ml DNase I for 30 min at 37°C. The lysed tissue was then passed through a ϕ40-μm cell strainer. The flow-through fraction was washed with phosphate-buffered saline (PBS) by centrifugation at 500×g for 5 min at 4℃. Cells were analyzed by flow cytometry.

Flow cytometry analysis

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After staining, cells suspended in PBS containing 3% FBS were analyzed and/or sorted with a FACS Aria IIu cell sorter (Becton Dickinson, Franklin Lakes, NJ). The following combinations of lasers and emission filters were used for the detection of fluorescence: for the fluorescence of BV510, a 405-nm laser and a DF530/30 filter (Omega Optical); for the fluorescence of FITC and Alexa 488, a 488-nm laser and a DF530/30 filter; for the fluorescence of PerCP/Cy5.5 and 7-AAD, a 488-nm laser and a DF695/40 filter (Omega Optical); for the fluorescence of PE, a 561-nm laser and a DF582/15 filter (Omega Optical); for the LIVE/DEAD Fixable Red Dead Cell Stain Kit, a 561-nm laser and a DF610/20 filter (Omega Optical); for the fluorescence of PE-Cy7, a 561-nm laser and a DF780/60 filter (Omega Optical); for the fluorescence of APC, a 633-nm laser and a DF660/20 filter (Omega Optical); and for the fluorescence of APC-Cy7, a 633-nm laser and a DF780/60 filter. Cells were first gated for size and granularity to exclude cell debris and aggregates, and dead cells were excluded by LIVE/DEAD Fixable Red Dead Cell Stain Kit or 7-AAD. Data analysis was performed using FlowJo software (Tree Star, Ashland, OR). For intracellular staining of Ly6G, isolated splenocytes were fixed and permeabilized with BD Cytofix/Cytoperm Fixation/Permeabilization Solution Kit (Thermo Fisher Scientific). Then, cells were incubated with anti-Ly6G antibody for 20 min at 4℃. Cells were washed twice with BD Perm/Wash Buffer and stained with FITC Goat anti-rat IgG antibody for 20 min at 4℃. Cells were washed three times with BD Perm/Wash Buffer and further stained with anti-CD11b antibody for 20 min at 4℃. After twice wash with BD Perm/Wash Buffer, cells were analyzed by flow cytometry as described above.

Instrumentation settings of bioluminescence imaging

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Bioluminescent images were acquired using a MIIS system (Molecular Devices, Japan, Tokyo) equipped with an iXon Ultra EMCCD camera (Oxford Instruments, Belfast, UK) and a lens (MDJ-G25F095, φ16 mm, F: 0.95; Tokyo Parts Center, Saitama, Japan). Images were acquired under the following condition: binning, 4; EM gain, 1000. For blocking of LFA-1, mice were injected with 100 μg of αLFA-1α antibody or an isotype control antibody, rat IgG2a, 2 hr before tumor injection. For MEK inhibition, mice were injected with PD0325901 i.p., 1 hr before and 8 hr after tumor injection. For vitamin K-dependent protease inhibition, mice were treated in their drinking water with 2.5–5 mg/L warfarin dissolved in an ethanol solution. Control mice were treated with the ethanol vehicle solution only. Solutions were prepared fresh every 3–4 days. The treatment started at least day –5 before tumor injection and continued until the end point of the experiment. For factor X or thrombin inhibition, mice were orally administrated with 20 mg/kg edoxaban or 330 mg/kg dabigatran etexilate twice a day. Prothrombin time was measured on blood samples collected from warfarin, edoxaban, and dabigatran etexilate-treated mice before starting experiment using CoaguChek XS system (Roche).

Bioluminescence imaging of lung metastasis

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B6 albino, BALB/c, or nude mice (female, 8–10 weeks old) were used in this experiment. Akaluc-expressing cells were suspended in PBS at 2×106 cells/ml, and 250 µl of the suspension was injected intravenously 60 min before imaging. Mice were anesthetized with 1.5% isoflurane (FujiFilm Wako Pure Chemical Corporation) inhalation and placed on a custom-made heating plate in the supine position. Immediately after the administration (i.p.) of 100 µl of 5 mM AkaLumine-HCl, bioluminescent images were acquired using a MIIS system (Molecular Devices, Japan, Tokyo). During the interval of long-term observation (more than 1 hr), mice were recovered from anesthesia and, immediately before observation, anesthetized again and administered AkaLumine as described. In some experiments, 4×105 B16F10 melanoma cells in 50 μl PBS containing 50% Geltrex (Thermo Fisher Scientific) were injected into the footpad of 6 weeks old female mice. After 2 weeks, B16-Akaluc cells were injected from tail vein. For serial injection, 5×105 B16-Akaluc cells were injected into the tail vein of mice that had been injected PBS or B16F10 cells into tail vein 24 hr before. For continuous observation of less than 3 hr, 100 µl of 15 mM AkaLumine-HCl was administered to the mice immediately after tumor injection. Acquisition of bioluminescent images was started at 5 min after tumor injection and repeated every 1 min. Image acquisition and analysis were carried out with MetaMorph software. The details of instrumentation settings and drug administration are summarized in Supplementary Methods.

Bioluminescence imaging of spontaneous lung metastasis

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BALB/c or nude mice were inoculated with 5×105 or 1×104 4T1-Akaluc cells suspended in 50 μl PBS containing 50% Geltrex at the footpad of right hind limb, respectively. Every 2–3 days, bioluminescence images were acquired immediately after the administration (i.p.) of 100 µl of 5 mM AkaLumine-HCl. To mask bioluminescence signals from the primary tumor site, right hind limb was covered with black silicon clay. Images were acquired under the following condition: binning, 4 no EM gain, exposure: 180 s. Image acquisition and analysis were carried out with MetaMorph software.

Instrumentation settings of two-photon excitation microscope and characterization of flowing and crawling NK cells

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Mice were observed with an FV1200MPE‐BX61WI upright 2P excitation microscope (Olympus, Tokyo, Japan) equipped with an XLPLN 25XW‐MP 25×/1.05 water‐immersion objective lens (Olympus) and an InSight DeepSee laser. Image areas of 500×500 µm2 to a depth of 25 µm were acquired every 30 s for 60–120 min, with Z steps at 2.5 µm. Images of 512×512 pixels were scanned at 2 μs/pixel with 1.0–1.2× digital zoom. The excitation wavelengths for cyan fluorescent protein, green fluorescent protein, and tdTomato were 840, 930, and 1040 nm, respectively. We used an IR‐cut filter, BA685RIF‐3 (Olympus), two dichroic mirrors, DM505 and DM570 (Olympus), and four emission filters, BA460‐500 (Olympus) for cyan fluorescent protein, BA495‐540 (Olympus) for green fluorescent protein, BA520‐560 (Olympus) for yellow fluorescent protein, and 645/60 (Chroma Technology Corp, Bellows Falls, VT) for tdTomato fluorescence. For the characterization of flowing and crawling NK cells, 1.5–2×106 B16-SCAT3 cells or B16-GCaMP cells were administered to NK-tdTomato mice through the tail veil. After 2 hr, images of a 0.25-mm2 FOV at a depth of 25 µm were acquired every 30 s for 2 hr. Crawling NK cells were defined as cells whose trajectory was recorded in more than four frames, that is 2 min, before contact with a melanoma cell. Flowing NK cells were defined as cells that were already in contact with the melanoma cells when they first appeared in the FOV. Cells were counted manually by using MetaMorph software. For imaging the signaling molecules activity in vivo, fluorescent images were acquired with three channels using the following filters and mirrors: an infrared (IR)-cut filter, BA685RIF-3, two dichroic mirrors, DM505 and DM570, and four emission filters, FF01-425/30 (Semrock, Rochester, NY) for the second-harmonic generation channel (SHG Ch), BA460-500 for the CFP Ch, BA520-560 for the FRET and GCaMP6s Ch. The excitation wavelength for CFP and GCaMP was 840 nm.

Intravital pulmonary imaging by two-photon excitation microscopy

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Lung intravital imaging was performed as described previously (Kamioka et al., 2017) with some modifications. In brief, mice were anesthetized by 1.5% isoflurane inhalation and placed in the right lateral position on an electric heating pad. The body temperature was maintained at 36°C using a heating pad with a BWT-100A rectal thermometer feedback controller (Bio Research Center, Nagoya, Japan). The mice were then anesthetized with 1.0% isoflurane supplied through a tracheostomy tube Surflo indwelling catheter 22G (Terumo, Tokyo, Japan) connected to an MK‐V100 artificial respirator (Muromachi Kikai, Tokyo, Japan). The respirator condition was as follows: O2 and air gas ratio, 80:20; beats per min, 55; gas flow, 35 ml/min; inspiratory/expiratory ratio, 3:2. The left lung lobe was exposed by 5th or 6th intercostal thoracotomy with custom-made retractors. A custom‐made vacuum‐stabilized imaging window was placed over the lung. Minimal suction (0.3–0.4 bar) was applied to stabilize the lung against the coverslip. All movies were median-filtered for noise reduction. Image analysis was carried out with Imaris (Bitplane, Belfast, UK) and MetaMorph software. The details of instrumentation settings and characterization of flowing and crawling NK cells are summarized in Supplementary Methods.

Tracking and motion analysis of NK cells in the lung

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For 3D tracking, time-lapse image areas of 500×500 µm2 and 25 µm thickness at a depth of 10–35 µm were acquired every 30 s. In some experiments, 1.5–2×106 B16-SCAT3 cells were intravenously injected and images were acquired for 2 hr after 4 hr after tumor injection. Image analysis was carried out with Imaris and MetaMorph software. Tracking of NK cells or tumor cells was performed by the 3D tracking function of Imaris. The time-series data of the coordinates were used to calculate track duration, length, speed, and displacement. The parameters of 3D tracking by Imaris were as follows: max distance, 30 μm; max frame gap, 2. We used the 3D position of traced cells for the motion analysis. The instantaneous speed v was calculated as the speed between two consecutive time frames, that is, v=rt-rt-Δt/Δt , where r is the position of cells, t is the elapsed time, and Δt is the time interval. We chose Δt=0.5 min. For Figure 3D–F, we ensembled all data over the cells and the elapsed time up to 50 min. The MSD of NK cells was calculated by the following equation: MSD=⟨|ri(t)−ri(0)|2⟩i , where ri is the position of cell i, and 〈〉 represents the average over cells. For the curve fitting in the MSD analysis, we used the nonlinear least-squares solver ‘lsqcurvefit,’ a built-in function of MATLAB (Mathworks Inc, Natick, MA) to determine the exponent parameter of the diffusivity. In general, the MSD adopts the asymptotic power-law form: MSD tα , where α is the degree of diffusive motion. The motion is classified as normal diffusion when α=1 but as anomalous diffusion otherwise (Krummel et al., 2016). An NK cell hit on a tumor is defined by the event when an NK cell comes within 10 µm of a tumor cell. The hit probability is obtained by dividing the total number of hit events by the sum of the observation period of each tumor cell. MATLAB scripts and the data sets are available from the source code file.

Visualization of signaling molecule activity in vivo

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To detect caspase activity and Ca2+ influx in tumor cells under a 2P microscope, 1.5–2.0×106 B16-SCAT3 cells, B16-GCaMP cells, or B16-GCaMP-tdTomato-CAAX cells with Tyr deficiency were administered to NK-tdTomato mice through the tail vein. After tumor injection, a 500×500 µm2 FOV at a depth of 25 µm was imaged every 30 s for 4–6 hr. For simultaneous observation of ERK activity in NK cells and Ca2+ influx in melanoma cells, 1.5–2.0×106 B16-GCaMP cells were administered to NK-ERK mice through the tail veil. After tumor injection, a 500×500 µm FOV at a depth of 25 µm was imaged every 30 s for 6 hr.

In vitro culture of NK cells

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NK cells were purified by negative selection from mice splenocytes with an NK cell isolation kit II (Miltenyi Biotec, Bergisch Gladbach, Germany) in accordance with the manufacturer’s instructions. The post-sort purity of NK cells (NK1.1+CD3−) was >95%. Purified NK cells were plated in 96-well U-bottomed plates (Thermo Fisher Scientific) in complete RMPI medium supplemented with the recombinant murine 1000 U/ml IL-2 (PeproTech, Rocky Hill, NJ) and cultured for 5 days. In some experiments, DNAM-1+ or DNAM-1− NK cells were purified by a FACS Aria Ⅱu on day 2, and further cultured for 3 days. The purity of each NK cell fraction was >98%.

Time-lapse imaging of in vitro killing of tumor cells

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B16-R-GECO cells with Tyr deficiency (2×104) were plated on a collagen-coated 96-well glass-base plate (AGC, Tokyo, Japan) and cultured for more than 6 hr to facilitate cell adhesion. Immediately after starting imaging with an epifluorescence microscope, 2×104 NK cells derived from hyBRET-ERK-NLS mice were added to the wells containing adherent target cells. The cells were imaged with an IX81 inverted microscope (Olympus) equipped with a UPlanSApo 40×/0.95 objective lens (Olympus), a PRIME scientific CMOS camera (Photometrics, Tucson, AZ), a Spectra-X light engine (Lumencor, Beaverton, OR), an IX2-ZDC laser-based autofocusing system (Olympus), a MAC5000 controller for filter wheels and XY stage (Ludl Electronic Products, Hawthorne, NY), and an incubation chamber (Tokai Hit, Fujinomiya, Japan). The filters and dichroic mirrors used for time-lapse imaging were as follows: for FRET imaging, an 430/24 (Olympus) excitation filter, an XF2034 (455DRLP) (Omega Optical, Brattleboro, VT) dichroic mirror, and FF01-483/32 (Semrock) and 535/30 (Olympus) for CFP and FRET, respectively. For Red fluorescent protein imaging, 572/35 (Olympus) excitation filters, 89006 (Chroma Technology Corp) and FF408/504/581/667/762-Di01 (Semrock) dichroic mirrors, and 632/60 (Olympus) emission filters, respectively. MetaMorph software was used for background noise subtraction and image analysis. Background intensities were determined by using an empty culture dish with the same amount of media. After background subtraction, the FRET/CFP ratio images were represented in the intensity-modulated display (IMD) mode. In the IMD mode, eight colors from red to blue were used to represent the FRET/CFP ratio, with the intensity of each color indicating the mean intensity of FRET and CFP channels. To track NK cells, the CFP images were analyzed by using the Fiji TrackMate plugin. From the x and y coordinates, the fluorescence intensity of each cell was isolated and the FRET/CFP ratio was calculated by MATLAB.

Counting of macroscopic lung metastasis

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Single-cell suspensions of B16-Akaluc cells (5×105) were injected intravenously into mice. The lungs were harvested on day 14 or 15, and tumor nodules were counted under a dissection microscope.

Flow cytometric analysis of disseminated tumor cells in the lungs

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1.5–2.0×106 B16-Akaluc cells were intravenously injected and single-cell suspension of the lung cells was generated after 24 hr as described above. The expression level of Necl5 was analyzed by FACS Aria IIu cell sorter. Data analysis was performed using FlowJo software.

Quantification of shedding of extracellular domain of Necl5 in the lung

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1.5–2.0×106 B16-Necl5-ScNeo cells were intravenously injected. Images were acquired after 4 hr or 24 hr by intravital pulmonary imaging with a 2P excitation microscope as described above. After 24 hr, moving to the other FOV without B16-Necl5-ScNeo cells and 1.0×106 B16-Necl5-ScNeo cells were newly injected from tail vein. Images of newly injected B16-Necl5-ScNeo cells were acquired with the same condition with the image acquisition of 24 hr. To examine the effect of anticoagulants, mice were orally administrated with 330 mg/kg dabigatran etexilate 1 hr before tumor injection. The intensity of mScarlet and mNeonGreen in the plasma membrane was isolated by using MetaMorph software and the mScarlet/mNeonGreen ratio was calculated.

In vitro protease digestion

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1.0×105 B16F10 cells or 293T cells were resuspended in serum-free RPMI and incubated for 3 hr at 37℃ with 100 µg/ml thrombin. The expression level of murine Necl5 was analyzed by FACS Aria IIu cell sorter. Data analysis was performed using FlowJo software.

Observation of thrombus in pulmonary capillaries

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1.5–2×106 B16-GCaMP-tdTomato-CAAX cells were administered to hyBRET-ERK-NES mice through the tail veil and images were acquired after 24 hr. During image acquisition, injuries on endothelial walls were generated by momentarily exposing a small area of the vessel wall to a laser of 70 mW power at 840 nm for up to 1 s. Image analysis was carried out with MetaMorph software.

Quantification and statistical analysis

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The statistical differences between the two experimental groups were assessed by Welch’s t-test unless otherwise indicated. Kaplan-Meier survival analyses were performed using MATLAB, and the log-rank test was used to determine significance.

Data availability

Imaging data are deposited at SSBD: database (https://doi.org/10.24631/ssbd.repos.2021.08.001).

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Decision letter

  1. Carla V Rothlin
    Senior and Reviewing Editor; Yale School of Medicine, United States

In the interests of transparency, eLife publishes the most substantive revision requests and the accompanying author responses.

[Editors' note: this paper was reviewed by Review Commons.]

https://doi.org/10.7554/eLife.76269.sa1

Author response

Reviewer #1 (Evidence, reproducibility and clarity (Required)):

The authors aimed to understand the control and the elimination of disseminated tumor cells by NK cells within the lung, their main question being how pulmonary NK cells are able to prevent tumor cells from colonization in the lung.

To dissect this question, Hiroshi Ichise and colleagues took advantage of the ultra-sensitive bioluminescence whole body imaging system combined with intravital two-photon microscopy technology involving genetically-encoded biosensors tumor or NK cells to explore the behavior and functional competences of NK cells in an experimental lung metastasis model.

First, the authors have monitored the fate of intravenously injected B16-Akaluc cells from 5 min to 10 days and observe that tumor cells decrease rapidly within the first 12-24 hours. In parallel, they performed asialoGM1+ and NK1.1+ cells depletion by injection of depleting anti-aGM1 and antiNK1.1 antibodies in order to see the involvement of these populations on the elimination of the disseminated tumor cells. They conclude that a rapid decrease of the tumor cells is mediated by NK cells. Consisting with this first data, the authors observe also the same early NK cells mediated impact on two other syngeneic mouse tumor cell lines : the BRAFV600E melanoma and the colon adenocarcinoma MC-38.

In a second part, the authors dissected NK cell dynamic behaviors in the pulmonary capillaries by taking advantage of the NKp46iCRExrosa26dtTomato mice where NKp46+ cells are fluorescents and performed 2P intravital imaging to follow the in situ the NKp46+ cells behavior. They could nicely observe that NK cells arrive from the capillaries and patrol on the lung epithelial cells in a stall-crawl-jump manner. Moreover, they also show that the attachment to the pulmonary capillaries is mediated by LFA-1. In the presence of B16F10 tumor model, they observe that NK cells stay longer in the capillaries and increase their duration time of crawling indicating that NK cells stay in contact longer with tumor cells.

The authors then explored the NK-mediated tumor killing in the lung by measuring tumor cell apoptosis using B16F10-SCAT3 cells (which leads to visualize caspase 3 activation) and Ca2+ influx in tumor cells expressing two Ca2+ sensors, GCaMP6s and R-GECO. They could observe casp3 activation but also Ca+ influx on tumor cells within few minutes after encountering NK cells. They also observe that evasion of NK cell surveillance is mediated by Nectin-5 and Nectin-2 expressed on tumor cells.

Then, they focus on NK cell activation by looking at ERK activation. To do so, they have isolated NK cells from Tg mice expressing a FRET-based ERK biosensor and performed in vitro killing assay against B16-R-GECO tumor cells but also in vivo experiments. For the in vivo experiments, they have developed reporter mice whose NK cells express the FRET biosensor for ERK. They observe that ERK-dependent NK cell activation contributes to the elimination of disseminated tumor cells within the first few hours but not after 24 hours. Indeed, theu observe that B16F10-Akaluc tumor cells are equally eliminated when injected 24 hrs after a first injection of B16F10 or PBS in mice. The authors concluded that tumor cell acquire the capacity to evade NK cell surveillance after 24 hrs rather than a hypothesis toward NK cells loose tumoricidal activity over time.

Finally, the authors have explored their last result on the potential tumor cell evasion of the NK cell surveillance. They show that this NK cell evasion is mediated by the shedding of cell surface NeCl-5. They next show that clivage of extracellular domain of NeCl-5 was mediated by thrombin in vitro and that anti-coagulation factors such as Warfarin, Edoxaban or Dabigatran Etexilate promote tumor elimination as observed by the bioluminescence experiments. This loss prevents the NK cell signaling needed for effective killing of tumor targets.

However, most of the results remain correlations and have not been formally demonstrated or miss controls.

B16F10 is a well-known and characterized NK cell target in a in vivo model so the first part is not really knew except the in situ behavior of NK cells within the lung capillaries. The new mechanism of thrombin-mediated shedding of NeCl-5 causing evasion from NK Cell surveillance is really concentrated on the last figure (Figure N{degree sign}6) and some supplemental experiments are mandatory and needed to really confirm this affirmation.

We deeply appreciate the reviewer’s effort to evaluate our work. The reviewer criticizes that the mechanism is well known except “the in situ behavior of NK cells within the lung capillaries.” Indeed, this is what we wish to show in our work. Nobody has ever seen how NK cells kill metastatic tumor cells in the lung. There is a big gap between in vitro tissue culture experiments and in vivo macroscopic counting of metastatic nodules. Most researchers do not even know when and where in the lung NK cells kill metastatic tumor cells. Live imaging is a powerful approach to address such questions.

Reviewer #1 (Significance (Required)):

There are several points to address to improve the significance of these data.

Major points:

1. A global point : 3 mice/group is to small to analyse and interprete data because of the heterogeneity of the mice. Mean +/- SEM have to represented instead of SD.

For the sake of animal welfare, researchers are asked to use minimal number of mice. Moreover, only one mouse can be observed in each imaging session, which takes several hours. In most experiments we performed two independent experiments with three mice each. We believe the number is appropriate for this type of experiment. In case of small number of samples, we think SD is better than SEM.

2. The authors used the well-known polyclonal anti-asialoGM1 Ab to deplete NK cells. AsialoGM1 is also expressed by ILC1, T, NKT and gd+T cells but also basophils (Trambley J et al., Asialo GM1(+) CD8(+) T cells play a critical role in costimulation blockade-resistant allograft rejection. JCI, 1999). The authors checked the involvement only for the basophils. They have to check the depletion of each of these populations specifically in the lung to assume that the depletion impact only the NK cells or they must change their conclusion on the entire manuscript and say that not only NK cells is responsible and involved in the control of the disseminated tumor cells but maybe also ILC1, NKT and or gd+T cells.

We obtained similar observations by using BALB/c nu/nu mice, which lack T cells (Figure 1D-1G). Therefore, we can exclude the contribution of NKT and γδT cells, which are absent in BALB/c nu/nu mice, in the acute phase (< 24 hrs) examined in this study. ILC1 is known to promote lung metastasis of B16F10 cells {Gao, 2017 #284}, neglecting its role in the protection of metastasis in the acute phase. These statements have been included in the result section with the reference.

(Lines 167) “The experiment with nu/nu BALB/c mice also excluded the involvement of NKT and γδ T cells, with which αAGM1 cross-reacts (Trambley et al., 1999). […] But, ILC1 is known to promote lung metastasis of B16F10 cells (Gao et al., 2017), suggesting that the effect of αAGM1 is primarily caused by the depletion of NK cells.”

3. Lines 133 to 136 : The authors say that they “did not observe any significant difference in the relative increase of the bioluminescence signal between the control and αAGM1-treated mice, implying that NK cells eliminate disseminated melanoma cells primarily in the acute phase (< 24 hrs) of lung metastasis”. Please comment because the depletion of asGM1+ cells impact also the growth of the tumor until 8 days (Figure 1B-E-G).

After 24 hrs, the slope of increment of bioluminescence intensity (BLI) did not change significantly betweenαAGM1-treated mice and control mice. In both mice, the doubling times of melanoma cells are approximately one day. We have included this statement for the clarity (line 139-142). Importantly, after 24 hrs, we did not observe any significant difference in the relative increase of the bioluminescence signal between the control and αAGM1-treated mice. In both mice, the doubling time of melanoma cells are approximately 1 day, implying that NK cells eliminate disseminated melanoma cells primarily in the acute phase (< 24 hrs) of lung metastasis.

(Lines 137) “In both mice, the doubling time of melanoma cells are approximately 1 day, implying that NK cells eliminate disseminated melanoma cells primarily in the acute phase (< 24 hrs) of lung metastasis.”

4. Figure S3A-B : The authors say that basophils express aGM1 so they performed basophils involvement on the elimination of B16F10 tumor cells with depleting aCD200R3 mab. They also checked the involvement of neutrophils and monocytes. They observed that basophils, neutrophils and monocytes are not involved on the B16F10 elimination. But what is the hypothesis to assess the role of neutrophils and monocytes ? Moreover, they did not explore Basophil roles in the other models including MC-38, BRAFV600E and 4T1 tumor cells.

We depleted neutrophils and monocytes because antibody-mediated removal of leukocytes could have non-specifically increased the survival of tumor cells. We wished to show the specificity of our approach. As for expanding the number of experiments with different cell lines, we are afraid but it is too much burden, considering the period required for the experiments and animal welfare.

(5a) Figure 1D : Missing control : the author must add the WT Balbc + a-AGM1 as control.

We performed the suggested experiment. Because this experiment was conducted as a distinct set of experiment, we moved the WT BALB/c data from Figure 1D to Figure S2C. Legend to figures have been modified accordingly.

We have rephrased the sentences as follows:

(Lines 147) “We extended this approach to other syngeneic mouse tumor cell lines: BrafV600E mutated melanoma cells (Dhomen et al., 2009), MC-38 colon adenocarcinoma cells (Rosenberg et al., 1986), and BALB/c mice-derived 4T1 breast cancer cells (hereinafter called 4T1-Akaluk).”

(5b) Lines 154 to 156 : the authors say that “T cell immunity does not contribute to tumor cell reduction” because tumor cells are eliminated in the nu/nu mice as efficiently as in the WT Balbc mice. This is not correct because they are looking in a window that correspond to innate immunity activation (up to 24 hrs) so they cannot talk about T cell immunity, the adaptive response will come more later around 8 days after.

Yes, we are focusing on the early phase of the rejection of metastatic tumor cells. We have rephrased the sentences as follows:

(Line 162) “T cell immunity does not contribute to tumor cell reduction in the acute phase of rejection (< 24 hrs).”

6) Line 159 : (refer to point #2) To affirm that NK cells is critical and involved in the elimination of the disseminated tumor, authors have to perform experiment in a model of NK cell deficiency. The most relevant nowadays is the NKp46ICRExrosa26DTA mice that are deficient in NK cells but also ILC1 cells. Indeed, the authors have used the NKp46iCre mice model for other questions.

As the reviewer stated, the contribution of NK cells in the rejection of metastatic tumors is very well known. Therefore, we would like to refrain from repeating the experiments by using other genetically modified mouse lines, which will take at least one year. We wish to emphasize again that the new findings of our paper are related to in vivo imaging.

(7a) Figure 2F : IC missing.

We have included the IgG2a control antibody in Figure 2F. Figure legend and the Materials and methods section have been modified accordingly.

(7b) Lines 181-182 : Authors conclude that the effect of anti-LFA-1 on NK cells adhesion to the pulmonary endothelial cells is mediated primarily by LFA-1. It is not totally true because it is partially mediated as observed in the Figure 2F. So authors should change their conclusion and precise that the involvement is partially mediated by LFA-1.

According to the reviewer’s suggestion, we have toned down the conclusion as follows:

(Lines 190) As expected, αLFA-1α, but not αMac-1, markedly reduced the number of NK cells on the pulmonary endothelial cells (Figure 2F), indicating that the adhesion of NK cells to the pulmonary endothelial cells is mediated at least partially by LFA-1.

8) Figure S5B-C-D and S7: The authors talk about tumor cell death. But they are analyzing Ca2+ influx in vitro so it is a little bit different from the cell death. I'm wondering how the cell death is measured especially in the Figure S5D and S7?

Under microscopes, apoptosis can be easily recognized by the appearance of blebs. We have modified the sentence and included a video (Video EV4) in the revised paper.

(Lines 232) “A surge of Ca2+ influx was observed only in cells that were doomed to die (Figure S5C and Video EV4). 98% of cells that exhibited Ca2+ influx died by apoptosis with blebbing (Figure S5D).”

9) Figure 4H and lines 232-233 : the authors conclude that “damage to tumor cells is dependent on the engagement of DNAM-1 on NK cells”. There is any experiment performed to affirm this point so the authors cannot maintain this conclusion. First, the authors only analyzed Ca2+ influx at a specific time point. So this result only show that Nectin-5 and/or Nectin-2 expressed by B16F10 is involved in the Ca2+ influx following NK cell contact but there is any data on DNAM-1 contribution. So, the role on the NK cells and specifically DNAM-1+ NK cells have not been addressed here. To answer to that question, the author have to perform in vivo model of engrafted WT vs NeCl-5/2 ko B16F10 in a WT vs DNAM1 deficient NK cells mouse model to ascertain the contribution of NeCl-5/2-DNAM-1 on NK cells. Moreover, survival curve and bioluminescent experiments would be very appreciated.

Re: The use of Ca2+ as a surrogate marker for cell death.

We showed that most, if not all, cells died after Ca2+ influx in vitro (Figure S5D). Due to the limitation of the observation period of in vivo imaging, we used Ca2+ influx as the surrogate marker of cell death. We stated the reason as follows:

(Lines 234) “With these in vitro data in hand, we used the surge of Ca2+ influx as the surrogate marker for apoptosis of metastatic melanoma cells in vivo.”

Re: Necl-5/Nectin-2 knockout B16F10 cells.

According to the suggestion, in these three months we worked hard to see whether we could find a condition in which, Necl-5-/- Nectin-2-/- B16F10 cells evade NK cell killing in the lung. We established several Necl-5-/- Nectin-2-/- B16F10 cells clones to see the effect. As anticipated, these Necl-5-/- Nectin2-/- B16F10 cell clones were less sensitive to IL2-stimulated NK cells in vitro (Figure S7G). However, in the bioluminescence assay we found that Necl-5-/-/Nectin-2-/- B16F10 cells disappeared as rapidly as the parent B16F10 cells (Figure S10). We confirmed that there is no other DNAM-1 ligand in Necl5-/-/Nectin-2-/- B16F10 cells by using recombinant DNAM-1 (Figure S7E) and that ERK activation in NK cells was not observed by these mutants (Figure S7F). In conclusion, our data is consistent with previous reports that examined the role of DNAM-1- Necl-5 interaction by using B16F10 cells. We have revised the result section to include the data and added a paragraph on the discrepancy between in vitro and in vivo observation.

(Lines 340)

“Finally, we examined if loss of Necl-5 and Nectin-2 on B16F10 cells cause NK cell evasion. The Necl5-/- Nectin-2-/- B16F10 cells survived more efficiently than wild type B16F10 cells from charge of the IL2-stimulated NK cells in vitro (Figure S7G). […] This observation agrees with previous note that DNAM-1- Necl-5 interaction is not the only mechanism of B16F10 rejection by NK cells in vivo (Gilfillan et al., 2008).”

(Lines 393)

“The discrepancy of the effect of Necl-5 and Nectin-2 knockout between in vitro and in vivo reflects the complexity of the mechanism of activation and cytotoxicity of NK cells (Figure S7G and Figure S10). […] Finally, the discrepancy could also be explained by the previous reports that TIGIT+ NK cells can eliminate Necl-5-/- cells in vivo by missing-self recognition due to the education via Necl-5 on the host cells (He et al., 2017) and the effect of education on degranulation does not last in cell culture with IL-2 (Pugh et al., 2019).”

Re: Use of DNAM1 deficient NK cells.

We have shown in vitro data with DNAM-1-negative NK cells in Figure S7D. This experiment was performed by sorting of DNAM-1-negative NK cells. I understand the importance of the experiment with the DNAM-1-deficient mice. But the introduction of another knockout mouse line cannot be performed easily. Instead, we have toned down the conclusion on the requirement of signaling from Necl-5/Nectin-2 to DNAM-1.

(Lines 244) “As anticipated, tumor Ca2+ influx was almost completely abolished in the Necl-5 and Nectin-2-deficient B16F10 cells (Figure 4H), suggesting that damage to tumor cells is dependent on the engagement of Necl-5 and/or Nectin-2 on melanoma cells.”

Revision of summary and abstract:

Because the data of Necl-5-/-/Nectin-2-/- B16F10 cells did not corroborate our proposal that DNAM1-dependent killing of B16F10 cells in vivo, we rephrased our title as follows. We intend to claim that the novelty of our work is in the functional visualization of NK cell killing of tumor cells. “Functional Visualization of NK Cell-mediated Killing of Metastatic Single Tumor Cells”.

10) Lines 253-254 : the authors talk about tumor apoptosis but they are looking at Ca2+ influx. So, they should change their conclusion or show killing experiment.

In Figure S7, we have shown that the sustained Ca2+ influx is a useful surrogate marker for apoptosis. We have included this information explicitly in the revised paper.

(Lines 232) “A surge of Ca2+ influx was observed only in cells that were doomed to die (Figure S5C); 98% of cells that exhibited Ca2+ influx died by apoptosis with blebbing (Figure S5D). With these in vitro data in hand, we used the surge of Ca2+ influx as the surrogate marker for apoptosis of metastatic melanoma cells in vivo.”

11) Figure 6 : the authors conclude that the trombin dependent shedding of Necl-5 causes evasion of NK cells surveillance. Moreover, all experiments are correlations and do not implicate in the same experiment Necl-5, DNAM-1+ NK cells and trombin or anti-coagulation factors. So, as in the comment #9, to adress this point, the authors should inject WT vs Necl-5 deficient B16F10-Akaluc into WT vs NK cell depleted mice and monitor the bioluminescence of the tumor cells within 24 hrs following injection of anti-coagulation factors as in the Figure 6H. Moreover, the monitoring of the survival curve and the number of the lung metastasis would be also very important and informative to really answer to this point.

Because we failed to see the difference between wild-type and Necl-5-/- Nectin-2-/- B16F10 cells in the in vivo bioluminescence assay, we did not perform this experiment. As already stated, IL2-stimulated NK cells recognize Necl-5 and Nectin-2-deficient B16F10 cells poorly with cytotoxicity reduced by over 40%. This 40% change may not be detected in vivo setup. Therefore, we have toned down our conclusion and suggested the presence of alternative pathway to eliminate tumor cells in the lung as already described.

Minor points:

1) Figure 2E: The authors assess the involvement of LFA-1 and MAC-1 on the NK cells attachment to the pulmonary endothelial cells. But there is other adhesion molecules that are known to be expressed by NK cells as for example CR4 (CD11c/CD18). So, the attachment of NK cells could be also due to this molecule.

We agree. This question is related to the Major point #6. We have toned down the sentence as already described.

2) Lines 190 to 197 : Authors should put this methodology part in the “material and method” in order to be more clear on the message they want to deliver.

According to the suggestion, we moved the description on normal and anomalous diffusive motion to the Method Section (Supplementary material line 382).

3) Line 228 : There is any hypothesis or explanation regarding the use of Necl5/Necl2 deficient B16F10. Why authors decided to go and explore this pathway ? Authors could add some transition sentence and explanation to help readers.

According to the suggestion, we have included following statement.

(Lines 240) “It is reported that DNAM-1 on NK cells contributes to the elimination of B16F10 melanoma cells”.

4) The author could performed the same experiment as in Figure S7D and assessed ERK activation of DNAM+ vs – NK cells against WT vs Necl-5/ Necl-2KO R-GEKO B16F10 cells.

We have performed the requested experiment as a part of reply to comment #9 (Figure S7G).

5) Line 283 : Thanks to reformulate the sentence. Check the figures associated with the text.

We have read through the paper and amended errors. We apology the mistakes.

Reviewer #2 (Evidence, reproducibility and clarity (Required)):

The authors use in vivo imaging techniques to investigate the killing of lung metastasis by NK cells. They demonstrate that the cleavage of CD155 may result in resistance of killing by NK cells and suggest that this could be an immune evasion mechanism of metastatic tumor cells.

Overall, the subject is highly relevant, and the in vivo imaging is an interesting and highly relevant technique. However, the message, that tumor cells escape the killing by NK cells by cleavage of CD155 is interesting, but not yet fully supported by the data.

We would like to thank the reviewer for the effort of evaluation our work and very useful comments. We spent these three months to consolidate the evidence to show that the cleavage of Necl-5/CD155 contributes to the resistance of tumor cells against NK cells, but we failed to obtain positive results, probably because of the presence of an alternative pathway(s). Therefore, we have toned down our conclusion and modified the title as follows. Because the data of Necl-5-/-/Nectin-2-/- B16F10 cells did not corroborate our proposal that DNAM1-dependent killing of B16F10 cells in vivo, we rephrased our title as follows. We intend to claim that the novelty of our work is in the functional visualization of NK cell killing of tumor cells.

“Functional Visualization of NK Cell-mediated Killing of Metastatic Single Tumor Cells”.

Major comments:

1. Figure 6: To support their main claim the authors would need to transfect the tumor cells with a CD155 mutant, which cannot be cleaved by Thrombin and show that these tumor cells can no longer escape NK cell-mediated killing. This experiment is straight forward and feasible. Another important experiment along this line would be the use the CD155/CD112 deficient tumor cells (Which the authors use in figure 4) in the experiments shown in figure 1. One would expect that tumor control by NK cells within the first 24 hrs is absent when using these tumor cells.

The potential thrombin cleavage site in Necl-5/CD155 is PRGSR (aa 129-133), wherein R/G is the cleavage site. We made 5 mutants, R130A, R130E, R130Q, G131W, and G131D. The G131W and G131D mutants were not detected by FACS, probably due to misfolding. The rest of 3 mutants were expressed as high as the WT Necl-5/CD155, DNAM-1+ NK cells failed to kill those mutants in vitro. Thus, it appears the recognition site by thrombin may also be critical for the binding to DNAM-1. Therefore, we were not able to conduct the requested experiment.

Re: Necl-5/Nectin-2 knockout B16F10 cells. Reviewer #1 raised a similar question; therefore, we repeat the same statement.

According to the suggestion, in these three months we worked hard to see whether we could find a condition in which, Necl-5-/- Nectin-2-/- B16F10 cells evade NK cell killing in the lung. We established several Necl-5-/- Nectin-2-/- B16F10 cells clones to see the effect. As anticipated, these Necl-5-/- Nectin2-/- B16F10 cell clones were less sensitive to IL2-stimulated NK cells in vitro (Figure S7G). However, in the bioluminescence assay we found that Necl-5-/-/Nectin-2-/- B16F10 cells disappeared as rapidly as the parent B16F10 cells (Figure S10). We confirmed that there is no other DNAM-1 ligand in Necl5-/-/Nectin-2-/- B16F10 cells by using recombinant DNAM-1 (Figure S7E) and that ERK activation in NK cells was not observed by these mutants (Figure S7F). In conclusion, our data is consistent with previous reports that examined the role of DNAM-1- Necl-5 interaction by using B16F10 cells. We have revised the result section to include the data and added a paragraph on the discrepancy between in vitro and in vivo observation.

(Lines 340)

“Finally, we examined if loss of Necl-5 and Nectin-2 on B16F10 cells cause NK cell evasion. The Necl5-/- Nectin-2-/- B16F10 cells survived more efficiently than wild type B16F10 cells from charge of the IL2-stimulated NK cells in vitro (Figure S7G). […] This observation agrees with previous note that DNAM-1- Necl-5 interaction is not the only mechanism of B16F10 rejection by NK cells in vivo (Gilfillan et al., 2008).”

(Lines 393)

“The discrepancy of the effect of Necl-5 and Nectin-2 knockout between in vitro and in vivo reflects the complexity of the mechanism of activation and cytotoxicity of NK cells (Figure S7G and Figure S10). […] Finally, the discrepancy could also be explained by the previous reports that TIGIT+ NK cells can eliminate Necl-5-/- cells in vivo by missing-self recognition due to the education via Necl-5 on the host cells (He et al., 2017) and the effect of education on degranulation does not last in cell culture with IL-2 (Pugh et al., 2019).

2. Figure 5: The demonstration that ERK is activated in this in vivo setting is novel. However, ERK activation is not DNAM-1 specific and the ERK inhibitor is significantly less effective that the depletion of NK cells. Therefore, the relevance of these data to the main message of the manuscript is unclear and the figure could be omitted.

We agree that the modest effect of MEKi implies that activation of the DNAM-1- ERK pathway is not the sole mechanism of tumoricidal activity of NK cells. Indeed, the result described above show that there is an alternative pathway(s) in vivo. However, we wish to emphasize that ERK activation is a useful marker of NK cell activation. The data shown here vividly show the timing of NK cell activation and following tumor cell killing. Because the in vivo dynamics of NK cell activation and tumor cell killing is the most important message of this work, we wish to show this data. We have modified the conclusion as follows:

(Lines 285) “Although interpretation is limited by the action of the soluble inhibitor on cells other than NK cells, these additional data are consistent with our imaging data and the idea that activated NK cell contributes to the elimination of disseminated tumor cells and that ERK activation can be used a marker for activated NK cells.”

3. In general, the issue of NK cell exhaustion should be addressed in more detail. The experiments do not address serial killing activity of NK cells and more data is needed to show that it is not an exhaustion of NK cells but the cleavage of CD155 from the tumor cells that prevents further killing.

We believe that NK cell exhaustion would not happen in a population level in this metastasis model by the following reason. There are 2.4 million NK cells in the lung and 1.0 million NK cells are replaced every minute (Supplementary Table). Therefore, NK cells outnumber 0.5 million melanoma cells injected into circulation. Moreover, each tumor cell in the lung is hit by an NK cell every two hours. Even if we assume that melanoma cells can inactivate NK cells every time, exhaustion of lung NK cells would not happen in 12 hours. Therefore, if NK cell exhaustion could happen, it should be mediated by indirect mechanism such as cytokine-induced suppression or endothelial cell-mediated inactivation etc. We have included these statements in the result section.

(Lines 304) “These results imply that NK cells in the lung are exhausted in 24 hrs. Our quantitative data shows that 2.4 million NK cells in the lung outnumber 0.5 million melanoma cells injected into circulation (Supplementary Table). Therefore, if NK cell exhaustion could happen, it is not caused by the killing of tumor cells, but by an indirect mechanism such as cytokine-induced suppression or endothelial cell-mediated inactivation.”

Figure 1C: The relevance of this experiment needs to be better explained.

We have modified the result section as follows:

(Lines 139) “In tumor burden mice, the lung microenvironment is often reprogrammed in favor of metastasis (Altorki, Markowitz et al., 2019). To test this possibility, B16F10 melanoma cells were inoculated into the foot pad two weeks prior to the intravenous injection of the B16-Akaluc cells (Figure 1C).”

2. Figure 3A: What does SHG stand for?

We have included the statement that SHG stands for second harmonic generation channel in the figure legend (Line 794).

3. Figure 3: Please add a statistical analysis for these experiments.

We have included P values in the Figure 3 of the revised paper.

4. Figure 4: The use of the caspase-3 and the calcium sensors may detect different cytotoxic mechanisms used by the NK cells. While caspase-3 can be activated by death receptor and perforin/granzyme B mediated killing, the calcium sensor may report mostly on perforin mediated membrane damage. These killing mechanisms have different kinetics and are differentially used during serial killing by NK cells. This should be addressed (at least in the discussion).

We thank this invaluable comment. We have included this point as follows:

(Lines 220) “During serial killing of tumor cells by NK cells, perforin/GrzB initially plays a major role, followed by Fas-mediated killing (Prager et al., 2019). Therefore, we used two biosensors to detect NK cell-mediated killing in vivo: SCAT-3 for Fas-mediated caspase activation and GCaMP-6s for the perforin/GrzB-mediated membrane damage.”

Reviewer #2 (Significance (Required)):

Investigating the in vivo cytotoxicity of NK cells against tumor cells by using live imaging technologies is highly relevant for the understanding of the dynamic relationship between tumor and killer cells. Therefore, the subject of this manuscript and the technologies used are very relevant, as in vivo killing activities do not always translate to the in vivo setting.

We thank the reviewer for the favorable comment.

Reviewer #3 (Evidence, reproducibility and clarity (Required)):

Summary:

Ichise et al., present a solid work describing the modality and time frame of action of NK control over seeding metastatic cells within the lung vasculature. Th authors use a variety of technique able to dissect how NK patrol lung vasculature, that they interact with cancer cells as they interact with the endothelial cells and they activate a ERK dependent activation leading to calcium influx in cancer cells leading to their death. The data support the notion that this NK control occur over an early time frame, 4h after cancer cells arrival and is mediated by Necl expression on cancer cells. After this time point cancer cells show a thrombin dependent loss of Necl expression on their surface and therefore become resistant to NK control.

Comments:

The data presented are supporting the conclusions. This work utilizes a variety of elegant strategy combining reporter strategy with in vivo imaging to assess the phenomenon of interaction, ERK activation, Calcium Inflax and Apoptosis activation directly in the lung.

In term of experiments, I found the work thorough and complete.

The data a presented well overall and the statistics seems adequate. I only have few suggestions:

We would like to thank the reviewer for the favorable comments.

Supplementary Figure S3, show the use of antiLy6G to deplete neutrophils in the lungs of C57BL/6 mice injected with melanoma B16F10 cells. It was recently shown that this antibody is not efficient in depleting neutrophils in this background, but only lead neutrophils to internalise the Ly6G so they cannot be detected by FACS. As shown in Boivin et al. 2020 http://doi.org/10.1038/s41467-020-165969) neutrophils depletion in C57BL/6 mice can be achieved by using antiGr1 antibody. Therefore, if the authors aim to show this additional control, which I also agree is really good to have, I suggest performing the experiment accordingly to the best-known practice.

According to the suggestion, we have examined intracellular Ly-6G (Figure S3E, lower panels) and found that it was decreased from 1.54% to 0.68%. So, we have toned down the effect of αLy-6G as follows:

(Lines 154) “Similarly, the roles of circulating monocytes and neutrophils were examined with clodronate liposome and αLy-6G neutrophil antibody, respectively. […] Although the effect of these reagent to eliminated monocytes and neutrophils was not complete, these data suggest the involvement of monocytes and neutrophils in the rejection of melanoma cells in the acute phase.”

Figure 1E: in the text the experiment is described as 4T1 Akaluc cells were inoculated into the foot pad of BALB/c mice with either control antibody or αAGM1, but the legend states that mice subcutaneously injected with B16 Akaluc cells into footpad. As B16 melanoma cells are not in BALB/c background, I assume the legend needs to be corrected as the cells should be 4T1, however I wonder if injecting 4T1 breast cancer cells in the footpad could have let to the substantial growth required for lung metastasis without impairing the animal mobility. Could it be that cells where actually injected in the fat pad of the mice and this is just a misspelling in the text?

We apology the erratum in the legend. We used 4T1-Akaluc cells in the experiment shown in Figure 1E, because 4T1 cells inoculated into footpad can be spontaneously metastasized to the lung (Kamioka et al., 2017). The legend has been amended accordingly.

(Lines 764) “€ BALB/c mice were pre-treated with either control antibody or αAGM1. Shown are representative merged images of the bright field and the bioluminescence images of mice subcutaneously injected with 5×105 4T1-Akaluc cells into footpad.”

In this case, the different in the tissue residence NK cells could also potentially explain why 4T1 are not cleared in the fat pad like the B6 cells are in the footpad.

We cannot neglect this possibility. But, the αAGM1 treatment did not affect the growth of the primary tumor as described (Figure 1F), suggesting that probably the effect of local NK cells is modest.

The authors should comment on the difference in the in clearance of the cells at the injection site in Figure 1C VS Figure 1E.

In both subcutaneous injection model, tumor cells at the injection site were not eliminated. Although we show it in the 4T1 subcutaneous injection model in Figure 1F but not in the B16F10 model. We have included the following sentence:

(Lines 142) “In this model, B16F10 melanoma cells continue to grow until at day 14 when B16Akaluc cells were further injected.”

Reviewer #3 (Significance (Required)):

The present work is highly relevant to the field of cancer metastasis. While it is known that NK are responsible for the first line of defence against metastatic seeding, most of the studies focuses on how they are suppressed or influenced by other immune cells. The present study provides a very accurate description of their mechanism of action, how they depend in the interaction with the endothelial cells and highlight the novel aspect of thrombin in inducing cancer cells NK resistance. What cause thrombin activation is the next relevant question, by in my opinion this study is complete and important.

My field of expertise is cancer metastasis and their interaction with the immune system and I personally enjoy very much reading this work.

We thank the reviewer for favorable comments and appreciate the effort to evaluate our work.

Other modifications:

1. Affiliation has been modified.

2. ORCID IDs have been updated.

3. Acknowledgement: We have referred to Dr. D. A. Russler-Germain, who provided comments (line 531).

4. Materials and methods: nectin cell adhesion molecule 2 (Nectin-2) was changed to Nectin-2. Line 499

5. Median was changed to mean. Line 221

6. A part of the Materials and methods section was moved to Supplementary Methods.

7. Materials and methods section was modified to fit the Author Checklist.

https://doi.org/10.7554/eLife.76269.sa2

Article and author information

Author details

  1. Hiroshi Ichise

    Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Kyoto, Japan
    Contribution
    Conceptualization, Data curation, Formal analysis, Funding acquisition, Investigation, Methodology, Writing - original draft
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5187-810X

  2. Shoko Tsukamoto

    Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Kyoto, Japan
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  3. Tsuyoshi Hirashima

    Department of Pathology and Biology of Diseases, Graduate School of Medicine, Kyoto University, Kyoto, Japan
    Contribution
    Data curation, Formal analysis, Writing - original draft
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-7323-9627

  4. Yoshinobu Konishi

    Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Kyoto, Japan
    Contribution
    Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-1212-7212

  5. Choji Oki

    Department of Nanopharmaceutical Sciences, Nagoya Institute of Technology, Gokiso-cho, Nagoya, Japan
    Contribution
    Methodology, Resources
    Competing interests
    No competing interests declared

  6. Shinya Tsukiji

    Department of Nanopharmaceutical Sciences, Nagoya Institute of Technology, Gokiso-cho, Nagoya, Japan
    Contribution
    Methodology, Resources, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-1402-5773

  7. Satoshi Iwano

    Brain Science Institute, Center for Brain Science, RIKEN, Hirosawa, Wako, Japan
    Contribution
    Methodology, Resources
    Competing interests
    No competing interests declared

  8. Atsushi Miyawaki

    Brain Science Institute, Center for Brain Science, RIKEN, Hirosawa, Wako, Japan
    Contribution
    Methodology, Resources, Writing - review and editing
    Competing interests
    No competing interests declared

  9. Kenta Sumiyama

    Laboratory for Mouse Genetic Engineering, RIKEN Center for Biosystems Dynamics Research, Suita, Japan
    Contribution
    Methodology, Resources, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-8785-5439

  10. Kenta Terai

    Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Kyoto, Japan
    Contribution
    Project administration, Supervision, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-7638-3720

  11. Michiyuki Matsuda

    1. Research Center for Dynamic Living Systems, Graduate School of Biostudies, Kyoto University, Kyoto, Japan
    2. Department of Pathology and Biology of Diseases, Graduate School of Medicine, Kyoto University, Kyoto, Japan
    3. Institute for Integrated Cell-Material Sciences, Kyoto University, Kyoto, Japan
    Contribution
    Conceptualization, Data curation, Formal analysis, Funding acquisition, Project administration, Supervision, Validation, Writing - review and editing
    For correspondence
    matsuda.michiyuki.2c@kyoto-u.ac.jp
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5876-9969

Funding

Japan Society for the Promotion of Science (18K15317)

  • Hiroshi Ichise

Japan Society for the Promotion of Science (15H05949)

  • Michiyuki Matsuda

Japan Society for the Promotion of Science (19H00993)

  • Michiyuki Matsuda

Japan Agency for Medical Research and Development (19gm5010003h0003)

  • Michiyuki Matsuda

Fugaku Trust for Medicinal Research

  • Michiyuki Matsuda

Core Research for Evolutional Science and Technology (JPMJCR1654)

  • Michiyuki Matsuda

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

The authors thank J Miyazaki, T Nagai (Osaka University), and M Miura (University of Tokyo) for the plasmids, T Setoyama, T Chiba (Kyoto University), and C Reis e Sousa (Francis Crick Institute) for the cell lines, M Yanagida (Kyoto University) for the mice, F Gochi (Kyoto University) for the intercostal thoracotomy, and R N Germain (NIAID), D A Russler-Germain (Washington University School of Medicine), and K Ikuta (Kyoto University) for the critical reading of this manuscript. The authors are grateful to the members of the Matsuda Laboratory for their helpful input, and to K Hirano, K Takakura, A Kawagishi, and Y Takeshita for their technical assistance. This work was supported by the Kyoto University Live Imaging Center. Financial support was provided by JSPS KAKENHI Grant nos. 18K15317 (to HI), 15H05949 (to MM), 16H06280 (to MM), and 19H00993 (to MM), AMED Grant no. 19gm5010003h0003 (to MM), Fugaku Trust for Medical Research (to MM), and JST CREST Grant no. JPMJCR1654 (to MM).

Ethics

The animal protocols were reviewed and approved by the Animal Care and Use Committee of Kyoto University Graduate School of Medicine (approval no. 19090).

Senior and Reviewing Editor

  1. Carla V Rothlin, Yale School of Medicine, United States

Publication history

  1. Preprint posted: January 17, 2021 (view preprint)
  2. Received: December 19, 2021
  3. Accepted: January 22, 2022
  4. Accepted Manuscript published: February 3, 2022 (version 1)
  5. Version of Record published: February 15, 2022 (version 2)

Copyright

© 2022, Ichise et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Hiroshi Ichise
  2. Shoko Tsukamoto
  3. Tsuyoshi Hirashima
  4. Yoshinobu Konishi
  5. Choji Oki
  6. Shinya Tsukiji
  7. Satoshi Iwano
  8. Atsushi Miyawaki
  9. Kenta Sumiyama
  10. Kenta Terai
  11. Michiyuki Matsuda
(2022)
Functional visualization of NK cell-mediated killing of metastatic single tumor cells
eLife 11:e76269.
https://doi.org/10.7554/eLife.76269

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